METHOD FOR PRODUCING A DEUTERATED OR TRITIATED NAD(P)H

Field of the invention

The present invention relates to methods for producing labelled cofactors comprising one or more Ή atom, wherein x is 2 or 3. The invention also relates to methods of producing labelled reaction products comprising one or more Ή atom derived from the labelled cofactor. The invention further relates to systems for the production of such labelled cofactors and labelled reaction products.

Background

Incorporation of deuterium ( ² H) into a molecule can induce changes to the kinetic, spectroscopic, mass and optical properties relative to the corresponding ('Hl-isotopologue. Accordingly, deuterated molecules are frequently utilised in chemical- and biochemical-mechanistic studies, with the deuterium kinetic isotope effect (DKIE), for example, often being employed to elucidate the rate-determining elements of multistep reactions. Recently, deuterated pharmaceuticals, long used in diagnostic studies, are being re-evaluated for previously overlooked DKIE-induced therapeutic properties, with a number of new drug companies synthesising only deuterium-labelled compounds.

Methods of incorporating ² H labels into molecules are known. For example, a common strategy is to employ a deuterated reducing agent such as LiAl( ² H)4 or NaB( ² H)4 to deliver a deuteride ( ² EF) anion to an oxidised carbon. However, such reagents are extremely expensive, frequently dangerously reactive, and typically react with little or no chemo-, regio- and/or stereo-selectivity.

Other known methods of incorporating ² H atoms into organic compounds include chemical‘hydrogenation’- type reactions, which have been used to add ² ¾ across double bonds. Such methods rely on the use of ² ¾ as the reductant, with the ² ¾ gas being activated by metal catalysts. However, such methods typically rely on the use of expensive metals such as platinum. Furthermore, the hydrogenation reaction typically requires conditions of high temperatures and high pressures, which are often impractical, prohibitively expensive and/or unsafe to use commercially. In addition, such hydrogenation reactions typically proceed with little or no selectivity, meaning that control of the final product and accurate distribution of the ² H label(s) can be unachievable. An alternative route to deuterated compounds involves catalysed H/D exchange. However, this strategy tends to lead to complete or near-complete deuteration of the compound, and is thus also unsuitable for selective labelling.

Various attempts to overcome the technical challenges of such chemical reaction routes have been made.

One approach that has been considered is to exploit the chemistry of biological cofactors such as nicotinamide adenine dinucleotide (NAD). Cofactors are non-protein chemical compounds that play an essential role in many enzyme catalysed biochemical reactions, and which typically act to transfer chemical groups between enzymes. In vivo, reduction of the oxidised cofactor (NAD ⁺ ) by hydride transfer from a reductant yields the reduced cofactor (NADH). The reduced cofactor can be coupled to enzymatic reduction of an oxidised centre (typically an oxidised carbon centre) to yield a reduced centre. Limited attempts have been made to reduce the oxidised cofactor using sources of ² H to yield [ ² H]-NADH, with a view to using the labelled reduced cofactor to reduce carbon centres in a selective manner. However, attempts to date have been largely unsuccessful.

One potential approach that has been considered relies on chemical reduction of the oxidised cofactor to generate Ή-labelled cofactor, wherein x is 2 or 3. However, such approaches have proven to be unsuccessful, as the use of the necessary chemical reductants tends to lead to generation of bio-inactive forms of the cofactor. Such methods thus cannot be used to efficiently generate reduced labelled products.

An alternative approach that has been considered relies on the enzymatic reduction of NAD ⁺ to [ ² H]-NADH. The oxidoreductase enzymes formate dehydrogenase, glucose dehydrogenase and alcohol dehydrogenase have all been considered for their abilities to abstract deuteride anions from labelled organic compounds (formate, glucose and ethanol, respectively), and to transfer the deuteride anions to NAD ⁺ to form [¾]- NADH. However, these methods are unsuited to being used commercially due to the very high price of the necessary reductant ( ² H-formate, ² H-glucose and ² H-ethanol, respectively). Such reactions also typically demand that the deuterated reducing equivalent be used in superstoichiometric quantities. Furthermore, the reactions are atomically inefficient. Accordingly, purification of the product is required to prevent contamination with waste oxidised reductant.

In a variation of such methods, some approaches have proposed the in situ generation of isotopically labelled reductants for subsequent use. For example, ² H-glyceraldehyde-3 -phosphate can be obtained by chemical exchange and tautomerisation of the ¾ compound in the presence of ² ¾0, with the enzyme glyceraldehyde- 3 -phosphate dehydrogenase being used to abstract the deuterium label from the ² H-glyceraldehyde-3- phosphate and transfer it to NAD ⁺ to form [ ² H]-NADH, which can subsequently be used in downstream reactions such as the reductive deuteration of pyruvate to ² H-lactate. Similarly, enzymes such as alanine racemase can be used to catalyse the non-selective chemical exchange of 'H-alanine to ² H-alanine in the presence of ² ¾0, before an amino acid dehydrogenase is used to abstract the deuterium label from the ² H- alanine and transfer it to NAD ⁺ to form [ ² H]-NADH, which again can subsequently be used in downstream reactions. Again, these methods have significant problems. The reactions are atomically inefficient.

Purification of the desired product is also required to prevent contamination with waste oxidised reductant; such reactants being typically toxic and/or reactive. Furthermore, especially in enzyme mediated systems the percentage of the ² H label incorporated into the co- factor is typically dependent on the proportions of the relative enzymes present, and cannot be controlled simply by controlling the percentage of the isotopic label in the aqueous solution. Accordingly, there is a pressing need for improved methods of generating Ή-labelled cofactors and Ή- labelled reaction products. There is specifically a need for methods that avoid the requirement for expensive or dangerously reactive chemical reagents; methods that offer selective labelling of the final reaction product; methods that allow selective reduction of oxidised carbon centres and/or that do not rely on the use of expensive labelled reductants. The present invention aims to address some or all of these problems.

Summary of the invention

The inventors have surprisingly found that it is possible to use Ή ⁺ ions in solution to enzymatically reduce an oxidised cofactor in the presence of an electron source. The inventors have found that it is possible to produce Ή-labelled cofactors and reaction products in an atom-efficient, clean process. The claimed methods differ from those previously described as the reductant which is oxidised to provide electrons need not be labelled with Ή in order to produce a reduced labelled cofactor comprising one or more Ή atom, or to produce a reduced labelled reaction product comprising one or more Ή atom. This has additional advantages in terms of reduced costs and ease of operation of the method. For example, the reductant which is oxidised to provide electrons need not be highly purified.

Accordingly, the invention provides a method of producing a reduced labelled cofactor comprising one or more Ή atom, wherein x is 2 or 3, wherein said method comprises:

i) providing a composition comprising (i) Ή ⁺ ions and (ii) an oxidised cofactor;

ii) transferring electrons from an electron source to a first polypeptide which is an

NADH:acceptor oxidoreductase or an NADPH: acceptor oxidoreductase or a functional derivative or fragment thereof; and

iii) contacting the Ή ⁺ ions and the oxidised cofactor with the first polypeptide thereby

reducing the oxidised cofactor to form a reduced labelled cofactor comprising one or more XH atoms.

This method is illustrated schematically in Figure 1.

The inventors have previously reported in WO 2013/050760 a co-factor regeneration system for regenerating cofactors such as NADH. The inventors demonstrated that electrons could be transferred to an oxidised cofactor to reduce it in a reversible manner, and demonstrated cycling of unlabelled ['HJ-NADH. However, whilst methods of cycling unlabelled ['HJ-NADH are known, the successful production of labelled cofactor is by no means trivial. For example, it was previously considered that the changes in over-potential requirements that arise from the use of labelled reactants would prevent the successful operation of methods involving labelled reactants. Kinetic isotope effects were also considered likely to impede the successful cycling of labelled cofactors due to variations in bond strength, leading to a diminished ability of finely tuned enzymes to activate bonds to Ή atoms or to mediate the transfer of Ή atoms or ions to and from cofactors. It was also previously believed that in order to generate Ή-labelled reduced cofactors, the reductant which is oxidised to extract electrons for use in the reduction reaction would necessarily have to be labelled with Ή itself. This general understanding was reinforced by analogy with the observation (discussed in more detail herein) that for metal-catalysed reductive insertion of deuterium into organic compounds such as cofactors, labelling of the ¾ gas reductant (i.e. use of ¾) is required to yield a labelled reduced cofactor. Whilst such reductants are not incompatible with the methods of the invention, the ability of the methods of the invention to operate with unlabelled reductants represents a significant advantage. Furthermore, the claimed method has been shown to be extremely efficient, even when non-labelled reductants are used as the source of electrons, thus representing a significant advantage over previously known methods. In addition, the methods of the invention have been found to yield biologically active reduced cofactors. These aspects of the invention represent a surprising finding of the present inventors.

The invention also provides a method of producing a reduced labelled reaction product comprising one or more Ή atom, wherein x is 2 or 3, wherein said method comprises producing a reduced labelled cofactor according to the invention, and

iv) contacting the reduced labelled cofactor and an oxidised reactant with at least one enzyme that is an NADH-dependent oxidoreductase or an NADPH-dependent oxidoreductase or a functional derivative or fragment thereof such that the enzyme selectively transfers an Ή atom from the reduced labelled cofactor to the oxidised reactant thereby producing a reduced labelled reaction product and an oxidised cofactor.

This method is illustrated schematically in Figure 2.

The invention further provides a system for performing a method of the invention, the system comprising: i) a composition comprising (i) Ή ⁺ ions wherein x is 2 or 3 ;

ii) an oxidised cofactor;

iii) an electron source; and

iv) a first polypeptide which is an NADH: acceptor oxidoreductase or an NADPH: acceptor oxidoreductase or a functional derivative or fragment thereof;

wherein the system is configured such that, in use, (a) electrons are transferred from the electron source to the first polypeptide and (b) Ή ⁺ ions and the oxidised cofactor are contacted with the first polypeptide so as to reduce the oxidised cofactor to form a reduced labelled cofactor comprising one or more Ή atoms.

In the methods of the invention, electrons are transferred from the electron source to the first polypeptide. Contacting of the first polypeptide with Ή ⁺ ions and an oxidised cofactor as defined herein results in the reduction of the oxidised cofactor by the electrons and Ή ⁺ ions to form a reduced labelled cofactor, with the reduction reaction catalysed by the first polypeptide. Subsequent re-oxidation of the reduced labelled cofactor by contact with an NAD(P)H-dependent oxidoreductase and an oxidised reactant (which is reduced to form a reduced labelled reaction product) reforms the oxidised cofactor which can undergo the cycle multiple times. The inventors have found that it is thus possible to exploit the extreme efficiency and high selectivity of enzymatic reactions to label cofactors and reaction products with Ή atoms, wherein x is 2 or 3, in a much more cost effective, safe, efficient and clean manner than has hitherto been possible. Importantly, the methods of the invention do not require the use of any exogenous“co-substrate” to mediate the transfer of Ή ⁺ ions to the oxidised cofactor; rather, the Ή ⁺ ions are contacted with the first polypeptide and are transferred directly from the composition in which they are contained, e.g. directly from ^x ¾0, to the first polypeptide, where they, together with the electrons transferred to the first polypeptide, form a reduced labelled cofactor.

Description of the sequence listing

SEQ ID NO: 1 - the amino acid sequence of the Ralstonia eutropha soluble hydrogenase diaphorase HoxF. SEQ ID NO: 2 - the amino acid sequence of the Ralstonia eutropha soluble hydrogenase diaphorase HoxU. SEQ ID NO: 3 - the amino acid sequence of the Ralstonia eutropha soluble hydrogenase diaphorase Hoxl. SEQ ID NO: 4 - the amino acid sequence of the flavoprotein (Fp) subcomplex of Bos taurus Complex 1, 51 kDa.

SEQ ID NO: 5 - the amino acid sequence of the flavoprotein (Fp) subcomplex of Bos taurus Complex 1, 24kDa.

SEQ ID NO: 6 - the amino acid sequence of the Ralstonia eutropha NAD+-dependent formate

dehydrogenase, diaphorase moiety (FdsB).

SEQ ID NO: 7 - the amino acid sequence of the Ralstonia eutropha NAD+-dependent formate

dehydrogenase, diaphorase moiety (FdsG).

SEQ ID NO: 8 - the amino acid sequence of the Rhodobacter capsulatus NAD+-dependent formate

dehydrogenase, diaphorase moiety (FdsB).

SEQ ID NO: 9 - the amino acid sequence of the Rhodobacter capsulatus NAD+-dependent formate

dehydrogenase, diaphorase moiety (FdsG)

SEQ ID NO: 10 - the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase I, gamma subunit.

SEQ ID NO: 11 - the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase I, beta subunit.

SEQ ID NO: 12 - the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase II, gamma subunit.

SEQ ID NO: 13 - the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase II, beta subunit.

SEQ ID NO: 14 - the amino acid sequence of the diaphorase moiety of Rhodococcus opacus SH, HoxF.

SEQ ID NO: 15 - the amino acid sequence of the diaphorase moiety of Rhodococcus opacus SH, HoxU. SEQ ID NO: 16 - the amino acid sequence of the diaphorase moiety of Allochromatium vinosum SH, HoxF. SEQ ID NO: 17 - the amino acid sequence of the diaphorase moiety of Allochromatium vinosum SH, HoxU. SEQ ID NO: 18 - the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina Hoxl F. SEQ ID NO: 19 - the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina Hoxl U. SEQ ID NO: 20 - the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina Hox2F. SEQ ID NO: 21 - the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina Hox2U. SEQ ID NO: 22 - the amino acid sequence of the diaphorase moiety of Synechocystis sp. PCC 6803 HoxF. SEQ ID NO: 23 - the amino acid sequence of the diaphorase moiety of Synechocystis sp. PCC 6803 HoxU. SEQ ID NO: 24 - the amino acid sequence of the diaphorase moiety of Synechococcus elongatus PCC 6301 HoxF.

SEQ ID NO: 25 - the amino acid sequence of the diaphorase moiety of Synechococcus elongatus PCC 6301 HoxU.

SEQ ID NO: 26 - the amino acid sequence of the diaphorase moiety of Hydrogenophilus thermoluteolus SH HoxF.

SEQ ID NO: 27 - the amino acid sequence of the diaphorase moiety of Hydrogenophilus thermoluteolus SH HoxU.

SEQ ID NO: 28 - the amino acid sequence of the ferredoxin-NADP+ reductase of Chlamydomonas

reinhardtii.

SEQ ID NO: 29 - the amino acid sequence of the ferredoxin-NADP+ reductase of Anabaena.

SEQ ID NO: 30 - the amino acid sequence of the Ralstonia eutropha soluble hydrogenase moiety (HoxH). SEQ ID NO: 31 - the amino acid sequence of the Ralstonia eutropha soluble hydrogenase moiety (HoxY). SEQ ID NO: 32 - the amino acid sequence of the Ralstonia eutropha membrane-bound hydrogenase moiety (HoxG).

SEQ ID NO: 33 - the amino acid sequence of the Ralstonia eutropha membrane-bound hydrogenase moiety (HoxK).

SEQ ID NO: 34 - the amino acid sequence of the Ralstonia eutropha membrane-bound hydrogenase moiety (HoxZ).

SEQ ID NO: 35 - the amino acid sequence of the Ralstonia eutropha regulatory hydrogenase moiety (HoxB). SEQ ID NO: 36 - the amino acid sequence of the Ralstonia eutropha regulatory hydrogenase moiety (HoxC). SEQ ID NO: 37 - the amino acid sequence of the Escherichia coli hydrogenase 1 (large subunit).

SEQ ID NO: 38 - the amino acid sequence of the Escherichia coli hydrogenase 1 (small subunit).

SEQ ID NO: 39 - the amino acid sequence of the Escherichia coli hydrogenase 2 (large subunit).

SEQ ID NO: 40 - the amino acid sequence of the Escherichia coli hydrogenase 2 (small subunit).

SEQ ID NO: 41 - the amino acid sequence of the Aquifex aeolicus hydrogenase 1 (large subunit).

SEQ ID NO: 42 - the amino acid sequence of the Aquifex aeolicus hydrogenase 1 (small subunit).

SEQ ID NO: 43 - the amino acid sequence of the Hydrogenovibrio marinus hydrogenase (large subunit). SEQ ID NO: 44 - the amino acid sequence of the Hydrogenovibrio marinus hydrogenase (small subunit). SEQ ID NO: 45 - the amino acid sequence of the Thiocapsa roseopersicina hydrogenase HupL. SEQ ID NO: 46 - the amino acid sequence of the Thiocapsa roseopersicina hydrogenase HupS.

SEQ ID NO: 47 - the amino acid sequence of the Alteromonas macleodii hydrogenase small subunit.

SEQ ID NO: 48 - the amino acid sequence of the Alteromonas macleodii hydrogenase large subunit.

SEQ ID NO: 49 - the amino acid sequence of the Rhodococcus opacus SH hydrogenase moiety HoxH.

SEQ ID NO: 50 - the amino acid sequence of the Rhodococcus opacus SH hydrogenase moiety HoxY.

SEQ ID NO: 51 - the amino acid sequence of the Allochromatium vinosum Membrane Bound Hydrogenase large subunit.

SEQ ID NO: 52 - the amino acid sequence of the Allochromatium vinosum Membrane Bound Hydrogenase small subunit.

SEQ ID NO: 53 - the amino acid sequence of the Desulfovibrio fructosovorans nickel-iron hydrogenase large subunit.

SEQ ID NO: 54 - the amino acid sequence of the Desulfovibrio fructosovorans nickel-iron hydrogenase small subunit.

SEQ ID NO: 55 - the amino acid sequence of the Clostridium pasteurianum iron-iron hydrogenase 1.

SEQ ID NO: 56 - the amino acid sequence of the Clostridium acetobutylicum iron-iron hydrogenase.

SEQ ID NO: 57 - the amino acid sequence of the Chlamydomonas reinhardtii iron-iron hydrogenase.

SEQ ID NO: 58 - the amino acid sequence of the Desulfomicrobium baculatum nickel-iron-selenium

hydrogenase large subunit.

SEQ ID NO: 59 - the amino acid sequence of the Desulfomicrobium baculatum nickel-iron-selenium

hydrogenase small subunit.

SEQ ID NO: 60 - the amino acid sequence of the Hydrogenophilus thermoluteolus SH moiety HoxH.

SEQ ID NO: 61 - the amino acid sequence of the Hydrogenophilus thermoluteolus SH moiety HoxY.

SEQ ID NO: 62 - the amino acid sequence of the Desulfovibrio vulgaris Nickel Iron hydrogenase Small subunit, pdb 1 H2A, Chain S.

SEQ ID NO: 63 - the amino acid sequence of the Desulfovibrio vulgaris Nickel Iron hydrogenase Large subunit, pdb 1 H2A, Chain L.

SEQ ID NO: 64 - the amino acid sequence of the Desulfovibrio gigas Periplasmic [NiFe] hydrogenase Small subunit.

SEQ ID NO: 65 - the amino acid sequence of the Desulfovibrio gigas Periplasmic [NiFe] hydrogenase Large subunit.

SEQ ID NO: 66 - the amino acid sequence of the Salmonella enterica serovar Typhimurium LT2 nickel-iron hydrogenase 5 Large subunit.

SEQ ID NO: 67 - the amino acid sequence of the Salmonella enterica serovar Typhimurium LT2 nickel-iron hydrogenase 5 Small subunit.

SEQ ID NO: 68 - the amino acid sequence of the Pyrococcus furiosus soluble hydrogenase alpha subunit.

SEQ ID NO: 69 - the amino acid sequence of the Ralstonia eutropha soluble hydrogenase moiety variant HoxH 164A. SEQ ID NO: 70 - the amino acid sequence of the Ralstonia eutropha soluble hydrogenase variant

HoxF_E341 A+D467 S.

SEQ ID NO: 71 - the amino acid sequence of the E. coli Mo-containing formate dehydrogenase (EcFDH-H). SED ID NO: 72 - the amino acid sequence of the Comamonas testosteroni PQQ and heme dependent ethanol dehydrogenase.

SEQ ID NO: 73 - the amino acid sequence of the Phanerochaete chrysosporium FAD and heme dependent Cellobiose dehydrogenase (FAD containing subunit).

SEQ ID NO: 74 - the amino acid sequence of the Phanerochaete chrysosporium FAD and heme dependent Cellobiose dehydrogenase (Heme containing subunit).

SEQ ID NO: 75 - the amino acid sequence of the Myricoccum thermophilum heme containing Cellobiose dehydrogenase.

SEQ ID NO: 76 - the amino acid sequence of the Acinetobacter calcoaceticus PQQ containing Glucose Dehydrogenase.

SEQ ID NO: 77 - the amino acid sequence of the Desulfovibrio gigas W-containing Formate Dehydrogenase alpha subunit.

SEQ ID NO: 78 - the amino acid sequence of the Desulfovibrio gigas W-containing Formate Dehydrogenase beta subunit.

Brief Description of the Figures

Figure 1 shows a schematic diagram of the production of reduced labelled cofactor in accordance with the methods of the invention.

Figure 2 shows a schematic diagram of the production of reduced labelled reaction product in accordance with the methods of the invention.

Figure 3 shows a schematic diagram of the extraction of electrons from a reductant via a second polypeptide and the use of such electrons in the production of reduced labelled reaction product in accordance with the methods of the invention.

Figure 4 shows a schematic diagram of the production of reduced labelled cofactor by oxidation of a reductant by a modular, multidomain or multicomponent protein or protein complex comprising both a first polypeptide and a second polypeptide, in accordance with the methods of the invention.

Figure 5 shows a schematic diagram of the transfer of electrons from an electron source to a first polypeptide via a mediator. Figure 6 shows a schematic diagram of how the methods of the invention can be used to generate a labelled oxidised cofactor from an unlabelled oxidised cofactor in accordance with the invention.

Figure 7 shows H NMR of (A) NADH; (B) [4R- ² H]-NADH and [45- ² H]-NADH. Spectra reproduced from Hirst et ah, Biochemistry 2013, 52, 4048-4055.

Figure 8 shows UV-VIS (A) and 'H-NMR (B) spectra demonstrating generation of reduced cofactor ([45- ² H]-NADH) from oxidised unlabelled cofactor (NAD ⁺ ) using methods of the invention wherein the electron source is E. coli hydrogenase 2 (SEQ ID NOs: 39-40) and the first polypeptide is R. eutropha soluble hydrogenase with an inactivated hydrogenase moiety (SEQ ID NOs: 1,2,31,69), and the first and second polypeptide are immobilized by adsorption onto carbon particles. Figure 8C shows an expanded region of the spectrum shown in Figure 8B confirming high ² H incorporation in the reduced cofactor. Data are described in Example 1A.

Figure 9 shows UV-VIS (A) and 'H-NMR (B) spectra demonstrating generation of reduced cofactor ([45- ² H]-NADH) from oxidised unlabelled cofactor (NAD ⁺ ) using methods of the invention wherein the electron source is E. coli hydrogenase 1 (SEQ ID NO: 37-38) and the first polypeptide is R. eutropha soluble hydrogenase with an inactivated hydrogenase moiety (SEQ ID NO: 1,2,31,69), and the first and second polypeptide are immobilized by adsorption onto carbon particles. Figure 9C shows an expanded region of the spectrum shown in Figure 9B confirming high ² H incorporation in the reduced cofactor. Data are described in Example IB.

Figure 10 shows UV-VIS (A) and 'H-NMR (B) spectra demonstrating generation of reduced cofactor ([45- ² H]-NADH) from oxidised unlabelled cofactor (NAD ⁺ ) using methods of the invention wherein the electron source is E. coli hydrogenase 2 (SEQ ID NOs: 39-40) and the first polypeptide is R. eutropha HoxF (SEQ ID NO: 1), and the first and second polypeptide are immobilized by adsorption onto carbon particles. Figure 10C shows an expanded region of the spectrum shown in Figure 10B confirming high ² H incorporation in the reduced cofactor. Data are described in Example 1C.

Figure 11 shows UV-VIS (A) and 'H-NMR (B) spectra demonstrating generation of reduced cofactor ([45- ² H]-NADH) from oxidised unlabelled cofactor (NAD ⁺ ) using methods of the invention wherein the electron source is the hydrogenase moiety of R. eutropha soluble hydrogenase (SEQ ID NOs: 30-31) and the first polypeptide is the diaphorase moiety of the R. eutropha soluble hydrogenase (SEQ ID NOs: 1-3) and the first and second polypeptides are component parts of a native enzyme complex. Figure 11C shows an expanded region of the spectrum shown in Figure 1 IB confirming high ² H incorporation in the reduced cofactor. Data are described in Example 2. Figure 12 shows UV-VIS (A) and 'H-NMR (B) spectra demonstrating generation of reduced cofactor ([45- ² H]-NADH) from oxidised unlabelled cofactor (NAD ⁺ ) using methods of the invention wherein the electron source is a carbon electrode and the first polypeptide is R. eutropha soluble hydrogenase with an inactivated hydrogenase moiety (SEQ ID NOs: 1,2,31,69) and the first polypeptide is adsorbed onto the carbon electrode. Figure 12C shows an expanded region of the spectrum shown in Figure 12B confirming high ² H incorporation in the reduced cofactor. Data are described in Example 3.

Figure 13 shows UV-VIS (A) and 'H-NMR (B) spectra demonstrating generation of reduced cofactor ([45- ² H]-NADPH) from oxidised unlabelled cofactor (NADP ⁺ ) using methods of the invention wherein the electron source is E. coli hydrogenase 2 (SEQ ID NOs: 39-40) and the first polypeptide is the soluble hydrogenase from R. eutropha (HoxHYFU, with D467S and E341A mutations in HoxF; SEQ ID NOs:

2,30,31,70), and the first and second polypeptide are immobilized by adsorption onto carbon particles.

Figure 13C shows an expanded region of the spectrum shown in Figure 13B confirming high ² H incorporation in the reduced cofactor. Data are described in Example 4.

Figure 14 shows schematic representations of methods investigated for generation of reduced labelled cofactor, [ ^X H]-NAD, from NAD ⁺ . All systems include a catalyst for ¾ oxidation and a NAD ⁺ reducing catalyst.

Pt/C = platinum supported on carbon;

Pt+NAD-R/C = platinum and NAD ⁺ reductase supported on carbon;

H2ase+NAD-R/C = hydrogenase and NAD ⁺ reductase supported on carbon;

soluble hydrogenase = unsupported soluble hydrogenase enzyme comprising both a first polypeptide and a second polypeptide as described herein.

Figure 15A shows HPLC spectra comparing the selectivity of the methods of the invention as described in Example 5. The traces show that the Pt/C system leads to significant generation of by-products. In contrast, systems utilizing NAD-R as the first polypeptide in accordance with the methods of the invention show high selectivity for 4-NADH. Figure 15B shows typical ¾ NMR data (400 MHz, 298 K) for such reactions. Results are described in Example 5.

Figure 16 shows an X-ray determined crystal structure of the NAD ⁺ binding site of Complex 1 from Thermus thermophilus ( Tt ) (PDB code: 3IAM; dark grey) and an overlay of a homology model of the R. eutropha HoxFU protein (SEQ ID NOs: 1,2; light grey) showing the corresponding NAD-R active site. Figure was generated using the standard software package PyMol. FMN and NADH cofactors are labelled - the FMN is underneath the NADH. The black dotted line denotes the distance between the atoms in FMN and NADH that the hydride is transferred between. The structure confirms that the hydride from FMN is delivered to the si face of the cofactor and confirms that electron transfer and proton transfer are decoupled by using NAD-R. Figure 17 shows a plot of ² H incorporation under a series of 'H ₂ 0: ² H ₂ 0 environments in (A) ¾ and (B) ² H ₂ gas following H ₂ -driven NAD ⁺ reduction by the Pt/C (dark grey, triangles);Pt+NAD-R /C (black, diamonds); and H2ase+NAD-R/C (light grey, squares) systems described in the Examples. The catalysts were removed prior to analysis by UV-vis spectroscopy and NMR. The dashed line is a line of best lit for the Pt+NAD-R/C system. Results are described in Example 6.

Figure 18 shows spectroscopic analysis of reactions in which labelled NADH is supplied to an NADH- dependent enzyme for chemo- and stereo-selective incorporation of at least one ² H atom. Using methods of the invention wherein the electron source is E. coli hydrogenase 2 (SEQ ID NOs: 39,40) and the first polypeptide is R. eutropha soluble hydrogenase with an inactivated hydrogenase moiety (SEQ ID NOs:

1,2,31,69), and the first and second polypeptide are immobilized by adsorption onto carbon particles, the labelled cofactor was continually recycled and supplied to (A) an 5-selective ADH, (B) an R-selective ADH, (C) an ene reductase and (D) an T-alanine dehydrogenase. The reaction products were analysed using either HPLC or GC and/or combination with 'H NMR. 'H NMR for analogous experiments in 'H ₂ 0 (control) and ¾ ₂ 0 (experiment) are shown. Only those in ² H ₂ 0 lead to labelled product. Experiments are described in Example 7.

Figure 18A (i): Chiral HPLC; (ii) 'H NMR

Figure 18B (i): Chiral HPLC; (ii) 'H NMR

Figure 18C (i): GC; (ii) 'H NMR

Figure 18D: 'H NMR

Figure 18E shows a summary of the reactions described in Example 7.

Figure 19 shows a reaction scheme demonstrating how the methods of the invention can be used to selectively generate [4.S- ² H]-NAD(P)H, [4R- ² H]-NAD(P)H, [4- ² H]-NAD(P)H and [4- ² H]-NAD(P) ⁺ .

Figure 20 shows UV-vis and 'H NMR spectroscopic results demonstrating the selective generation of [45- ² H]-NADH, [4R- ² H]-NADH, [4- ² H]-NADH and [4- ² H]-NAD ⁺ using methods of the invention. Experiments are described in Example 8.

Figure 21 shows results characterizing the products from the reductive deuteration of pyruvate using the methods of the invention. The results are compared to isotopically unenriched commercial lactate standards and a control reaction without the system of the invention present. (a)(i) Reaction scheme showing the derivatization of lactate for analysis by (a)(ii) GC-FID. (b)(i) Reaction scheme showing the diastereotopic derivatization of lactate for analysis by (b)(ii) GC-FID. (b) Mass spectra (El, 70 eV) and (c) 'H NMR analysis ( ² H ₂ 0, p ² H 8.0, 500 MHz, 293 K) of T-lactate produced in the deuteration reaction compared to an isotopically unenriched standard (d) Determined distribution of ² H labels across the product T-lactate. Results are described in Example 9.1. Figure 22 shows results characterizing the products from the reductive deuteration of phenylpyruvate using the methods of the invention. The results are compared to isotopically unenriched commercial phenylalanine standards and a control reaction without the system of the invention present. (a)(i) Reaction scheme showing the derivatization of phenylalanine for analysis by (a)(ii) GC-FID. (b)(i) Reaction scheme showing the derivatization of phenylalanine for analysis by (b)(ii) chiral-GC-FID. (c) Mass spectra (El, 70 eV) and (d) ¾ NMR analysis ( ² ¾0, p ² H 8.0, 500 MHz, 293 K) of T-phenylalanine produced in the deuteration reaction compared to an isotopically unenriched standard. Results are described in Example 9.2.

Figure 23 shows results characterizing the products from the reductive deuteration of cinnamaldehyde using the methods of the invention. In each case the results are compared to an isotopically unenriched commercial cinnamyl alcohol standard (a) GC-FID determination of the cinnamyl alcohol produced compared to cinnamaldehyde, cinnamyl alcohol standards and a control reaction (with no bio system added) showing that only a single product is made in each reaction with no side product formation (b) ¾ NMR analysis ( ² ¾0, p ² H 8.0, 500 MHz, 293 K) of the cinnamyl alcohol produced shows that high ² H incorporation is achieved.

(c) Mass spectra (El, 70 eV) of the cinnamyl alcohol produced compared to an isotopically unenriched standard. Results are described in Example 9.3 (reaction A).

Figure 24 shows results characterizing the products from the reductive deuteration of cinnamaldehyde using the methods of the invention. In each case the results are compared to an isotopically unenriched commercial hydrocinnamaldehyde standard (a) GC-FID determination of the cinnamyl alcohol produced compared to cinnamaldehyde, hydrocinnamaldehyde standards and a control reaction (with no bio-system added) showing that only a single product is made with no side product formation (b) ¾ NMR analysis ( ² ¾0, p ² H 8.0, 500 MHz, 293 K) of the hydrocinnamaldehyde produced shows that high ² H incorporation is achieved (c) Mass spectra (El, 70 eV) of the hydrocinnamaldehyde produced compared to the isotopically unenriched standard. Results are described in Example 9.3 (reaction B).

Figure 25 shows results characterizing the products generated using a two-step, one pot reductive deuteration reaction in accordance with the methods of the invention, with (i) an ene reductase acting on cinnamaldehyde and (ii) and alcohol dehydrogenase acting on the intermediate hydrocinnamaldehyde. In each case the results are compared to an isotopically unenriched commercial 3 -phenyl- 1 -propanol standard (a) GC-FID determination of the 3 -phenyl- 1 -propanol produced compared to cinnamaldehyde, hydrocinnamaldehyde and 3 -phenyl- 1 -propanol standards and a control reaction (with no bio- system added) showing that only a single product is made in each reaction with no side product formation (b) ¾ NMR analysis ( ² ¾0, p ² H 8.0, 500 MHz, 293 K) of the 3 -phenyl- 1 -propanol produced shows that high ² H incorporation is achieved (c) Mass spectra (El, 70 eV) of the 3-phenyl-l -propanol produced compared to the isotopically unenriched standard.

(d) Determined distribution of ² H labels. Results are described in Example 9.3 (reaction C). Figure 26 shows results characterizing the products from the reductive deuteration of (4R)-carvone by using the heterogeneous bio-system with an ene reductase. In each case the results are compared to an isotopically unenriched commercial dihydrocarvone standard, or a sample prepared by supplying an ene reductase with substrate and super-stoichiometric NADH. (a) GC-FID determination of the dihydrocarvone produced compared to standards and a control reaction (with no bio-system added) (b) ¾ NMR analysis ( ² ¾0, p ² H 8.0, 500 MHz, 293 K) and (c) Mass spectra (El, 70 eV) of the dihydrocarvone produced from the reaction . Results are described in Example 9.4 (reaction A).

Figure 27 shows results characterizing the products from the reductive deuteration of (45)-carvone by using the heterogeneous bio-system with an ene reductase. In each case the results are compared to an isotopically unenriched dihydrocarvone samples, prepared by zinc reduction of the carvone or by supplying the ene reductase with substrate and super-stoichiometric NADH. (a) GC-FID determination of the dihydrocarvone produced compared to standards and a control reaction (with no bio-system added) (b) ¾ NMR analysis ( ² H ₂ 0, p ² H 8.0, 500 MHz, 293 K) and (c) Mass spectra (El, 70 eV) of the dihydrocarvone produced from the reaction compared to isotopically unenriched samples. Results are described in Example 9.4 (reaction B).

Figure 28 shows that the methods of the invention can be used in selective reductive tritiation of reactants such as acetophenone (a) 1H NMR analysis of product confirms (> 80 %) acetophenone was converted to 1 -phenylethanol. (b) Liquid scintillation calibration allowed the radioactivity of the extracted product sample to be determined. Results are described in Example 10.

DETAILED DESCRIPTION OF THE INVENTION

Methods of the invention

As described above, the invention provides methods for producing reduced labelled reaction products comprising one or more Ή atom, wherein x is 2 or 3. In such methods, the oxidised cofactor produced in step (iv) of the method is preferably re-reduced to form a reduced labelled cofactor in accordance with the methods described herein. Preferably, the reduced labelled reaction product thus produced is subsequently oxidised and reduced multiple times in methods of the invention, thereby recycling the cofactor.

For avoidance of doubt, by recycling the cofactor, it is meant that a single cofactor molecule can be reduced in a method of the invention to form a reduced labelled cofactor. The reduced labelled cofactor can subsequently transfer a labelled hydrogen atom to an oxidised reactant to yield a reduced labelled reaction product and an oxidised cofactor, which can be re-reduced as described. The repeated reduction and oxidation of the cofactor corresponds to recycling of the cofactor. The net result is that the cofactor itself is not consumed, and the Ή ⁺ ions and electrons are consumed by the oxidised reactant in the production of reduced labelled reaction product. This method is illustrated schematically in Figure 2.

In methods of the invention which involve recycling the cofactor, each cofactor molecule is typically recycled as defined herein at least 10 times, such as at least 100 times, more preferably at least 1000 times e.g. at least 10,000 times or at least 100,000 times, such as at least 1,000,000 times. Accordingly, in methods of the invention, the turnover number (TN) is typically at least 10, such as at least 100, more preferably at least 1000 e.g. at least 10,000 or at least 100,000, such as at least 1,000,000. As those skilled in the art will appreciate, the TN indicates the number of moles of product generated per mole of cofactor, and is thus a measure of the number of times each cofactor molecule is used.

Enzyme turnover can be calculated in a number of ways. The Total Turnover Number (TTN, also known as the TON) is a measure of the number of moles of product per mole of enzyme (specifically per mole of the first polypeptide). Accordingly, in methods of the invention for the production of a reduced labelled cofactor, the TTN indicates the number of moles of reduced labelled cofactor generated per mole of first polypeptide. As those skilled in the art will appreciate, the TTN thus indicates the number of times that the enzyme (i.e. the first polypeptide) has turned over.

The Turnover Frequency (TOF) is a measure of the number of moles of product generated per second per mole of enzyme (first polypeptide) present. Accordingly, in methods of the invention for the production of a reduced labelled cofactor, the TTN indicates the number of moles of reduced labelled cofactor generated per second per mole of first polypeptide. Accordingly, the TOF is identified with the number of catalytic cycles undertaken by each enzyme molecule per second.

Preferably, in the methods of the invention, the first polypeptide has a TOF of 0.1 to 1000 s ¹ , more preferably 1 to 100 s ¹ such as from about 10 to about 50 s ¹ .

The composition comprising Ή ⁺ ions and oxidised cofactor typically comprises ² ¾0 or ³ H2q as the source of ^x H ⁺ ions; typically the composition further comprises substances such as buffers and the like, as described herein, in addition to the oxidised cofactor itself. Typically, therefore, the Ή ⁺ ions are provided as ² ¾0 or ³ H ₂ 0. Those skilled in the art will appreciate that when the composition comprising Ή ⁺ ions comprises both Ή2O and ¾0, the Ή ⁺ ions may be present in the form of 'HΉO. Those skilled in the art will appreciate that Ή ⁺ ions can be present in the form of hydrogen-containing compounds or in the form of solvated ions e.g. ^x H ⁺ _(aq) e.g. ^x ¾0 ⁺ , ¹ ff2 ^x ffO ⁺ or ¹ H ^X H ₂ 0 ⁺ . Even at neutral or alkaline pH (p ^x H) a non-zero concentration of ^x H ⁺ _(aq) ions are present in aqueous solution. Of course, the composition comprising Ή ⁺ ions and oxidised cofactor may also comprise reduced cofactor, oxidised reactant and/or reduced labelled reaction product according to the methods of the invention. It will be apparent that as used herein, labelled organic molecules such as glucose, formate, and ethanol are not sources of Ή ⁺ ions.

Most preferably, the Ή ⁺ ions are provided as ² ]¾0. The compositions of the invention can comprise unlabelled water (H2O) or can be free of H2O. Preferably, when the Ή ⁺ ions used in the methods of the invention are ² H ⁺ ions, the ratio of ² H ⁺ to H ⁺ ions (i.e. H2O) is at least 1:99, such as at least 10:90, more preferably at least 20:80 e.g. at least 50:50 such as at least 80:20, more preferably at least 90: 10 e.g. at least 95:5 such as at least 99: 1. Preferably, when the Ή ⁺ ions used in the methods of the invention are ² H ⁺ ions, the composition comprising (i) Ή ⁺ ions is free or essentially free of H2O (e.g. less than 0.1% or less than 0.01% H2O); i.e. when ² H ⁺ ions are used in the methods of the invention, the composition preferably comprises large amounts of ² H ⁺ ions.

In the methods of the invention, the concentration of Ή ⁺ ions in the composition comprising Ή ⁺ ions can be controlled to produce reduced labelled cofactor and/or labelled reaction product in the desired percentage purity. For example, for some applications it is desirable to produce reduced labelled cofactor or reduced labelled reaction product wherein the label is present at ppm levels, i.e. where the amount of reduced labelled cofactor or reduced labelled reaction product is from about 0.00001% to about 0.01%, such as from about 0.0001% to about 0.001%, relative to the amount of the unlabelled cofactor or product. In other applications it is desirable to produce reduced labelled cofactor or reduced labelled reaction product wherein the labelled cofactor or product is present in larger amounts, such as in amounts of from 1% to 100%, such as from 10% to about 99% e.g. from about 40% or about 50% to about 95% or about 90%, relative to the amount of the unlabelled cofactor or product. The extremely high efficiency of the reactions employed in the methods of the invention allow this to be controlled with accuracy by controlling the amount of Ή ⁺ ions in the composition comprising Ή ⁺ ions. For example, if it is desired to produce reduced cofactor wherein 10% of the reduced cofactor is labelled with Ή, this can be achieved by the use of a composition comprising 10%

Ή ⁺ ions relative to the total number of H ⁺ ions in the concentration.

For example, when it is desired to produce reduced labelled cofactor or reduced labelled reaction product wherein the label is present at ppm levels as described above, this can be achieved by use of a composition comprising Ή ⁺ ions in an amount of from about 0.00001% to about 0.01%, such as from about 0.0001% to about 0.001%, relative to the total amount of H ⁺ ions in the concentration. Preferably, when ³ H ⁺ ions are used in the methods of the invention, the composition comprises ppm levels of ³ H ⁺ ions.

In the methods of the invention, any cofactor that can be reduced by an NADFhacceptor oxidoreductase or an NADPFhacceptor oxidoreductase or a functional derivative or fragment thereof as defined herein can be used. Preferably, the cofactor is nicotinamide adenine dinucleotide or nicotinamide adenine dinucleotide phosphate. More preferably, the cofactor is nicotinamide adenine dinucleotide. Nicotinamide adenine dinucleotide exists in the oxidised form (NAD ⁺ ) and the reduced form (NADH). Similarly, nicotinamide adenine dinucleotide phosphate exists in the oxidised form (NADl^) and the reduced form (NADPH). The oxidized forms NAD ⁺ and NADP ⁺ act as electron acceptors, by being reduced. NADH and NADPH, in turn, can act as reducing agents, by being oxidized. Those skilled in the art will appreciate that the term NAD(P)H refers to either NADH or NADPH. The term NAD(P) ⁺ refers to either NAD ⁺ or NADP ⁺ . The structures of NAD ⁺ and NADP ⁺ are shown below:

NAD ⁺ , showing the 4- position of the nicotinamide NADP ⁺ , showing the 4- position of the nicotinamide ring ring

As described herein, the methods of the invention comprise reduction of an oxidised cofactor. Preferably, the reduction involves adding an Ή atom at the 4- position of the nicotinamide ring of the oxidised cofactor, as shown below. (The 4- position of the nicotinamide ring in NAD ⁺ and NADP ⁺ is indicated above).

The 4- position of the nicotinamide ring in NAD ⁺ and NADP ⁺ comprises a hydrogen atom. In NAD ⁺ and NADP ⁺ , that hydrogen atom is typically ¾ However, the methods of the invention are not limited to methods wherein the hydrogen atom at the 4- position of the nicotinamide ring is ¾ but also embrace those methods wherein the hydrogen atom at the 4-position of the nicotinamide ring of the oxidised cofactor is ² H or ³ H. In other words, in the methods of the invention, the oxidised cofactor is NAD ⁺ , NADP ⁺ , or a labelled version of NAD ⁺ or NADP ⁺ comprising at least one Ή atom, typically wherein the Ή atom is at the 4- position of the nicotinamide ring.

The methods of the invention can be used to generate both stereoisomers of the singularly labelled reduced cofactor, the doubly labelled reduced cofactor and the labelled oxidised cofactor; i.e. [45- ^x H]-NAD(P)H, [4 R- ^X H]-NAD(P)H, [4- ^X H ₂ ]-NAD(P)H and [4- ^x H]-NAD(P) ⁺ . As used herein, the term [4S- ^X H]-NAD(P)H refers to the reduced form of NAD(P)H wherein the carbon atom at the 4-position of the nicotinamide ring is bonded to a ³ H atom and an Ή atom and wherein the absolute stereochemistry at that carbon position is S, as defined by the Cahn-Ingold-Prelog rules. As used herein, the term [4/?- ^x H]-NAD(P)H refers to the reduced form of NAD(P)H wherein the carbon atom at the 4-position of the nicotinamide ring is bonded to a ³ H atom and an Ή atom and wherein the absolute stereochemistry at that carbon position is R, as defined by the Cahn- Ingold-Prelog rules. As used herein, the term [4- ^x H ₂ ]-NAD(P)H refers to the reduced form of NAD(P)H wherein the carbon atom at the 4-position of the nicotinamide ring is bonded to two Ή atoms. As used herein, the term [4- ^x H]-NAD(P) ⁺ refers to the oxidised form of NAD(P)H wherein the carbon atom at the 4- position of the nicotinamide ring is bonded to one Ή atom. Preferably, in the methods of the invention, the oxidised cofactor is NAD ⁺ or NADP ⁺ . Most preferably, the oxidised cofactor is NAD ⁺ . Accordingly, the invention also provides methods for producing an oxidised labelled cofactor comprising an Ή atom, wherein x is 2 or 3, comprising producing a reduced labelled cofactor comprising one or more Ή atom according to the methods of the invention; and oxidising the reduced labelled cofactor thus produced.

The methods of the invention involve transferring electrons from an electron source to a first polypeptide which is an NADH:acceptor oxidoreductase or an NADPH: acceptor oxidoreductase or a functional derivative or fragment thereof, and contacting Ή ⁺ ions and oxidised cofactor with the first polypeptide thereby reducing the oxidised cofactor to form a reduced labelled cofactor comprising one or more Ή atoms.

Those skilled in the art will appreciate that contacting Ή ⁺ ions and oxidised cofactor with the first polypeptide involves the direct contact of the Ή ⁺ ions with the first polypeptide and the direct transfer of said Ή ⁺ ions to the first polypeptide. In other words, the Ή ⁺ ions are transferred directly from the composition in which they are contained (e.g. directly from Ή ₂ 0, e.g. directly from ² H ₂ 0 or ³ H ₂ 0) to the first polypeptide. The transfer of the Ή ⁺ ions to the first polypeptide is a consequence of the contacting of the Ή ⁺ ions with the first polypeptide. As explained above, labelled organic molecules such as glucose, formate, and ethanol are not sources of Ή ⁺ ions as used herein. As such, those skilled in the art will appreciate that Ή ⁺ ions are not transferred to the first polypeptide by contacting the first polypeptide by such labelled organic molecules. Furthermore, the invention does not involve the abstraction of Ή ⁺ ions from such labelled organic molecules, irrespective of whether such labelled organic molecules are provided exogenously or generated in situ, e.g. by chemical exchange with Ή2O. Thus, the methods of the invention do not involve the use of labelled organic molecules as co-substrates to mediate the transfer of Ή ⁺ ions from the composition in which they are contained (e.g. directly from ¾0, e.g. directly from ² ]¾0 or ³ ]¾0) to the first polypeptide.

Preferably, therefore, in the invention, contacting the Ή ⁺ ions and the oxidised cofactor with the first polypeptide comprises directly transferring an Ή ⁺ ion to the first polypeptide. Preferably, contacting the Ή ⁺ ions and the oxidised cofactor with the first polypeptide comprises directly transferring an Ή ⁺ ion directly from Ή2O, e.g. directly from ² ]¾0 or ³ ]¾0) to the first polypeptide. Preferably, contacting the Ή ⁺ ions and the oxidised cofactor with the first polypeptide comprises directly transferring an Ή ⁺ ion directly from Ή2O, e.g. directly from ² ]¾0 or ³ ]¾0) to the first polypeptide without transferring an Ή ⁺ ion to an organic molecule (i.e. to a co-substrate). Preferably, the methods of the invention do not comprise contacting the first polypeptide with a labelled organic reactant containing an Ή atom. Preferably, the methods of the invention do not comprise transferring an Ή ⁺ ion from Ή2O (e.g. from ² ]¾0 or ³ ]¾0) to an organic molecule (i.e. to a co-substrate). Preferably, the methods of the invention do not comprise transferring an Ή ⁺ ion from an organic molecule (i.e. a co-substrate) to the first polypeptide. In other words, the methods of the invention preferably do not comprise using a labelled organic molecule as a co-substrate to mediate the transfer of Ή ⁺ ions from the composition in which they are contained (e.g. from Ή2O, e.g. from ² ]¾0 or ³ H ₂ 0) to the first polypeptide.

Accordingly, the invention preferably provides a method of producing a reduced labelled cofactor comprising one or more Ή atom, wherein x is 2 or 3, wherein said method comprises:

i) providing a composition comprising (i) Ή ⁺ ions and (ii) an oxidised cofactor;

ii) transferring electrons from an electron source to a first polypeptide which is an NADH:acceptor oxidoreductase or an NADPH:acceptor oxidoreductase or a functional derivative or fragment thereof; and iii) contacting the ^X H ⁺ ions and the oxidised cofactor with the first polypeptide, thereby directly transferring an Ή ⁺ ion to the first polypeptide, and thereby reducing the oxidised cofactor to form a reduced labelled cofactor comprising one or more Ή atoms.

Preferably, said method is a method of producing a reduced labelled reaction product comprising one or more Ή atom, wherein x is 2 or 3, and said method comprises producing a reduced labelled cofactor as defined herein; and

iv) contacting the reduced labelled cofactor and an oxidised reactant with at least one enzyme that is an NADH-dependent oxidoreductase or an NADPH-dependent oxidoreductase or a functional derivative or fragment thereof such that the enzyme selectively transfers an Ή atom from the reduced labelled cofactor to the oxidised reactant thereby producing a reduced labelled reaction product and an oxidised cofactor.

As described herein in more detail, such methods preferably further comprise reducing the oxidised cofactor produced in step (iv) in a method of the invention. Such methods may likewise comprise producing a reduced labelled reaction product according to steps (i) to (iv), and repeating steps (ii) to (iv) multiple times, thereby recycling the cofactor.

In the methods of the invention, any suitable NADH:acceptor oxidoreductase or NADPH:acceptor oxidoreductase or functional derivative or fragment thereof can be used as the first polypeptide. An NADH:acceptor oxidoreductase or NADPH:acceptor oxidoreductase or functional derivative or fragment thereof can be referred to as a diaphorase or diaphorase moiety.

As used herein, a NADH:acceptor oxidoreductase is a polypeptide capable of catalysing the reduction of NAD ⁺ to NADH. As used herein, a NADPH: acceptor oxidoreductase is a polypeptide capable of catalysing the reduction of NADP ⁺ to NADPH. It will be apparent to the skilled person that an NAD(P)H: acceptor oxidoreductase may either be a single polypeptide or may comprise multiple polypeptides, e.g. additional peptides in addition to the NAD(P)H: acceptor oxidoreductase. The NAD(P)H: acceptor oxidoreductase may also be a portion such as one or more domains of a multidomain polypeptide.

The first polypeptide preferably transfers an Ή anion (wherein x = 2 or 3) to the oxidised cofactor thereby forming the reduced labelled cofactor. Without being bound by theory, it is believed that the Ή ion is transferred to the oxidised cofactor in a concerted“two electron, one Ή ⁺ ” process, the two electrons and single proton combining to form an Ή anion. The two electrons and single proton are believed to be typically transferred by a cofactor such as a flavin cofactor contained in the first polypeptide. However, as those skilled in the art will appreciate the precise mechanism by which the Ή ion is transferred to the oxidised cofactor is immaterial to the efficacy of the overall process.

Preferably, the first polypeptide comprises a cofactor such as a flavin group. Preferably, the flavin group is an FAD (flavin adenine dinucleotide) or FMN (flavin mononucleotide) group.

Preferably, the structure of the first polypeptide is suitable for binding nucleotides such as NAD(P) ⁺ or NAD(P)H. A preferred structural motif for binding such nucleotides is the Rossmann fold. The Rossmann fold can be considered as a super-secondary structural motif characterized by alternating beta strand / alpha helix / beta strand secondary structures. Typically, Rossmann folds comprise up to four a helices and a sheet typically comprising 6 b strands. Proteins comprising Rossmann folds are well known to those skilled in the art.

Preferably, the first polypeptide comprises or consists of a diaphorase moiety. Diaphorases are a ubiquitous class of flavin-containing enzymes that typically catalyze the reduction of various dyes which act as hydrogen acceptors from NADH and NADPH. Diaphorases can be obtained from bacteria, plants and animals. Any suitable diaphorase capable of reducing an oxidised cofactor as defined herein in the presence of electrons and Ή ⁺ ions can be used in the methods of the invention. Preferably, the first polypeptide comprises or consists of one or more than one of:

i) the amino acid sequence of Ralstonia eutropha diaphorase HoxF (SEQ ID NO: 1) or an amino acid sequence having at least 60% homology therewith;

ii) the amino acid sequence of Ralstonia eutropha diaphorase HoxU (SEQ ID NO: 2) or an amino acid sequence having at least 60% homology therewith;

iii) the amino acid sequence of Ralstonia eutropha diaphorase Hoxl (SEQ ID NO: 3) or an amino acid sequence having at least 60% homology therewith;

iv) the amino acid sequence of the 51 kDa protein of the flavoprotein (Fp) subcomplex of Complex I of Bos taurus (SEQ ID NO: 4) or an amino acid sequence having at least 60% homology therewith;

v) the amino acid sequence of the 24kDa subcomplex of Complex I of Bos taurus (SEQ ID NO: 5) or an amino acid sequence having at least 60% homology therewith;

vi) the amino acid sequence of Ralstonia eutropha NAD ⁺ -dependent formate dehydrogenase diaphorase moiety FdsB (SEQ ID NO: 6) or an amino acid sequence having at least 60% homology therewith;

vii) the amino acid sequence of Ralstonia eutropha NAD ⁺ -dependent formate dehydrogenase diaphorase moiety FdsG (SEQ ID NO: 7) or an amino acid sequence having at least 60% homology therewith;

viii) the amino acid sequence of Rhodobacter capsulatus NAD ⁺ -dependent formate dehydrogenase, diaphorase moiety FdsB (SEQ ID NO: 8) or an amino acid sequence having at least 60% homology therewith;

ix) the amino acid sequence of Rhodobacter capsulatus NAD ⁺ -dependent formate dehydrogenase, diaphorase moiety FdsG (SEQ ID NO: 9) or an amino acid sequence having at least 60% homology therewith;

x) the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase I gamma subunit (SEQ ID NO: 10) or an amino acid sequence having at least 60% homology therewith;

xi) the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase I beta subunit (SEQ ID NO: 11) or an amino acid sequence having at least 60% homology therewith;

xii) the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase II gamma subunit (SEQ ID NO: 12) or an amino acid sequence having at least 60% homology therewith;

xiii) the amino acid sequence of the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase II beta subunit (SEQ ID NO: 13) or an amino acid sequence having at least 60% homology therewith; xiv) the amino acid sequence of the diaphorase moiety of Rhodococcus opacus soluble hydrogenase HoxF (SEQ ID NO: 14) or an amino acid sequence having at least 60% homology therewith; xv) the amino acid sequence of the diaphorase moiety of Rhodococcus opacus soluble hydrogenase HoxU (SEQ ID NO: 15) or an amino acid sequence having at least 60% homology therewith; xvi) the amino acid sequence of the diaphorase moiety of Allochromatium vinosum soluble

hydrogenase HoxF (SEQ ID NO: 16) or an amino acid sequence having at least 60% homology therewith;

xvii) the amino acid sequence of the diaphorase moiety of Allochromatium vinosum soluble

hydrogenase HoxU (SEQ ID NO: 17) or an amino acid sequence having at least 60% homology therewith;

xviii) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina HoxlF (SEQ ID NO: 18) or an amino acid sequence having at least 60% homology therewith;

xix) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina soluble

hydrogenase HoxlU (SEQ ID NO: 19) or an amino acid sequence having at least 60% homology therewith;

xx) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina Hox2F (SEQ ID NO: 20) or an amino acid sequence having at least 60% homology therewith;

xxi) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina soluble

hydrogenase Hox2U (SEQ ID NO: 21) or an amino acid sequence having at least 60% homology therewith;

xxii) the amino acid sequence of the diaphorase moiety of Synechocystis sp. PCC 6803 HoxF (SEQ ID NO: 22) or an amino acid sequence having at least 60% homology therewith;

xxiii) the amino acid sequence of the diaphorase moiety of Synechocystis sp. PCC 6803 HoxU (SEQ ID NO: 23) or an amino acid sequence having at least 60% homology therewith;

xxiv) the amino acid sequence of the diaphorase moiety of Synechococcus elongatus PCC 6301 HoxF (SEQ ID NO: 24) or an amino acid sequence having at least 60% homology therewith;

xxv) the amino acid sequence of the diaphorase moiety of Synechococcus elongatus PCC 6301 HoxU (SEQ ID NO: 25) or an amino acid sequence having at least 60% homology therewith; xxvi) the amino acid sequence of Hydrogenophilus thermoluteolus diaphorase HoxF (SEQ ID NO:

26) or an amino acid sequence having at least 60% homology therewith;

xxvii) the amino acid sequence of Hydrogenophilus thermoluteolus diaphorase HoxU (SEQ ID NO:

27) or an amino acid sequence having at least 60% homology therewith;

xxviii) the amino acid sequence of Chlamydomonas reinhardtii Ferredoxin-NADP+ reductase (SEQ ID NO: 28) or an amino acid sequence having at least 60% homology therewith;

xxix) the amino acid sequence of Anabaena Ferredoxin-NADP+ reductase (SEQ ID NO: 29) or an amino acid sequence having at least 60% homology therewith;

xxx) the amino acid sequence of Ralstonia eutropha diaphorase HoxF (SEQ ID NO: 70) or an amino acid sequence having at least 60% homology therewith; xxxi) the amino acid sequence of Ralstonia eutropha diaphorase with inactive hydrogenase (SEQ ID NO: 1 and/or 2 and/or 69 and/or 31) or an amino acid sequence having at least 60% homology therewith or a functional fragment, derivative or variant thereof.

One or more of the amino acid sequences described in (i) to (xxxi) above can be used as the first polypeptide.

When the first polypeptide comprises a variant of SEQ ID NO: 1, the variant may comprise point mutations such that the variant comprises one or more of the following mutations: i) K, S, A, N, R or H at position 326; more preferably, the variant comprises D326K;

ii) K, S, A, N, R or H at position 401; more preferably, the variant comprises D401K;

iii) K, S, A, N, R or H at position 467; more preferably, the variant comprises D467S;

iv) K, S, A, N, R or H at position 340; more preferably, the variant comprises D340A; and/or v) K, S, A, N, R or H at position 341 ; more preferably, the variant comprises E341 A or H341.

The above mutations are complementary and can be combined, for example, when the first polypeptide is a variant of SEQ ID NO: 1, the variant may preferably comprises D340A and E341A; D340A and D401K; D326K and D401K; D467S and D401K; D340N and D467S; and/or E341A and D467S. Without being bound by theory, it is believed that such variants can accommodate the additional negatively charged phosphate group of NADP ⁺ resulting in improved affinity and/or oxidation and/or reduction activity due to reduced negative charge around the NADP ⁺ binding site.

The first polypeptide preferably comprises or consists of the amino acid sequence of Ralstonia eutropha soluble hydrogenase moiety HoxF (SEQ ID NO: 1) or an amino acid sequence having at least 60% homology therewith. The first polypeptide can optionally further comprise the amino acid sequence of Ralstonia eutropha soluble hydrogenase moiety HoxU (SEQ ID NO: 2) or an amino acid sequence having at least 60% homology therewith. Accordingly, the first polypeptide may comprise or consist of the amino acid sequence of Ralstonia eutropha soluble hydrogenase moieties HoxFU (SEQ ID NOs: 1,2) or amino acid sequences having at least 60% homology therewith.

When the first polypeptide comprises the amino acid sequence of Ralstonia eutropha soluble hydrogenase moiety HoxF (SEQ ID NO: 1) or an amino acid sequence having at least 60% homology therewith, and optionally the amino acid sequence of Ralstonia eutropha soluble hydrogenase moiety HoxU (SEQ ID NO:

2) or an amino acid sequence having at least 60% homology therewith, the first polypeptide may optionally further comprise the amino acid sequence of Ralstonia eutropha soluble hydrogenase moieties HoxH and/or HoxY (SEQ ID NOs: 30,31) or amino acid sequences having at least 60% homology therewith. Without being bound by theory, it is believed that the presence of a HoxHY component in the first polypeptide increases the stability of the NADH:acceptor oxidoreductase or NADPH:acceptor oxidoreductase moiety leading to increased efficiency and/or activity. Many suitable methods for increasing the stability of proteins/ protein complexes are known in the art and may be used in the methods of the present invention.

Preferably, therefore, the first polypeptide comprises a HoxHYFU tetramer. More preferably, the first polypeptide comprises the HoxHYFU tetramer of Ralstonia eutropha (SEQ ID NOs: 1,2,30,31), or an amino acid sequence having at least 60% homology therewith. Still more preferably, the first polypeptide comprises the HoxHYFU tetramer of Ralstonia eutropha wherein the HoxH moiety is a non-functional variant, preferably comprising the point mutation I64A (SEQ ID NO: 69), or a sequence having at least 60% homology therewith (in which case the HoxH moiety comprises the point mutation I64A). HoxHYFU constructs comprising the I64A point mutation in the HoxH moiety are also known as HoxHYFU or NAD-R (SEQ ID NOs: 1,2,31,69).

Preferably, when the first polypeptide comprises or consists of one or more amino acid sequences having at least 60% homology with a specified sequence, each amino acid sequence independently has at least 70%, such as at least 80%, more preferably at least 90%, e.g. at least 95%, preferably at least 97%, such as at least 98%, preferably at least 99% homology with the specified sequence. More preferably, each amino acid sequence independently has at least 70%, such as at least 80%, more preferably at least 90%, e.g. at least 95%, preferably at least 97%, such as at least 98%, preferably at least 99% identity with the specified sequence. For avoidance of doubt, if the first polypeptide comprises two or more amino acid sequences, the percentage homology of each of the two or more sequences with respect to their respective specified sequences can be the same or different. Percentage homology and/or percentage identity are each preferably determined across the length of the specified sequence.

Variants ofNADHacceptor oxidoreductase or NADPH: acceptor oxidoreductases are also suitable for use as the first polypeptide in the methods of the present invention. For example, the first polypeptide may preferably be modified to have an increased catalytic activity for reducing the oxidised cofactor or oxidising the reduced cofactor as compared to the native enzymes. Preferably, variants have increased catalytic activity as compared to the activity of the Ralstonia eutropha diaphorase HoxF or HoxFU moieties (SEQ ID NOs 1,2). Preferably, the catalytic activity is at least 2 times, such as at least 5 times, e.g. at least 10 times, such as at least 100 times, preferably at least 1000 times the catalytic activity of the Ralstonia eutropha diaphorase HoxF or HoxFU moieties.

Catalytic activity can be determined in any suitable method. For example, the catalytic activity can be associated with the Michaelis constant K _M (with increased activity being typically associated with decreased K _M values) or with the catalytic rate constant, _cat (with increased activity being typically associated with increased k _{c at} values). Measuring K _M and k _cat is routine to those skilled in the art. For example, the K _M of the first polypeptide for a reduced cofactor can be determined spectrophotometrically by measuring absorption at 578 nm under anaerobic conditions at 30 °C in 50 mM Tris-HCl buffer, pH 8.0, containing 1 mM reduced cofactor, 5 mM benzyl viologen (oxidized; e = 8.9 mM ^-1 cur ¹ ), 90 mM dithionite, and 10 to 30 pmol of enzyme. Alternatively, the K _M of the first polypeptide for oxidised cofactor can be determined

electrochemically, by adsorbing the first polypeptide onto a pyrolytic graphite electrode immersed in an electrochemical cell containing buffered electrolyte (eg 50 mM phosphate at pH 7.0) and holding the electrode at a constant potential of -412 mV vs a standard hydrogen electrode while the concentration of the oxidised cofactor is increased by injection into the solution. The intercept on the (substrate concentration) axis of a plot of (substrate concentration)/(current magnitude) vs (substrate concentration) is equal to (-KM) (Lauterbach et al, PLoS ONE; doi: 10.1371/joumal.pone.0025939). The intercept on the (substrate concentration)/ (current magnitude) axis of such a plot is equal to ¾i/V _max with V _max = _cat [E] where [E] is the amount of enzyme present, which can typically be determined by integrating the background-subtracted redox peak observed for the enzyme in the absence of substrate.

More preferably, the first polypeptide consists or comprises of the Ralstonia eutropha NAD ⁺ -reducing soluble hydrogenase or a functional fragment, derivative or variant thereof. Still more preferably, the first polypeptide consists or comprises of the R. eutropha HoxF moiety (SEQ ID NO: 1) and optionally the HoxU diaphorase moieties (SEQ ID NO: 2) or an amino acid sequence having at least 60% homology (e.g. at least 70%, such as at least 80%, more preferably at least 90%, e.g. at least 95%, preferably at least 97%, such as at least 98%, preferably at least 99% homology) therewith. More preferably the first polypeptide consists or comprises of the HoxHYFU tetramer of Ralstonia eutropha (SEQ ID NOs: 1,2,30,31), or an amino acid sequence having at least 60% homology (e.g. at least 70%, such as at least 80%, more preferably at least 90%, e.g. at least 95%, preferably at least 97%, such as at least 98%, preferably at least 99% homology) therewith. Most preferably, the first polypeptide comprises HoxHYFU (also referred to herein as NAD-R, i.e. the HoxHYFU tetramer of Ralstonia eutropha wherein the HoxH moiety comprises the point mutation I64A (SEQ ID NOs: 1,2,31,69)), or a sequence having at least 60% homology (e.g. at least 70%, such as at least 80%, more preferably at least 90%, e.g. at least 95%, preferably at least 97%, such as at least 98%, preferably at least 99% homology) therewith (wherein the HoxH moiety comprises the point mutation I64A).

In the methods of the invention, the electron source preferably comprises a second polypeptide capable of oxidising a reductant to extract electrons (as illustrated in Figure 3); a synthetic organic, inorganic or metallic oxidation catalyst capable of oxidising a reductant to extract electrons; or an electrode connected to an electrode controller.

Preferably, the reductant is an organic compound such as formate, glucose, an alcohol, or the like, or is hydrogen (i.e. ¾ or ^x ¾ or mixtures thereof). Where the reductant is other than hydrogen, preferably the reductant is unlabelled. In one embodiment, the reductant is unlabelled. More preferably, the reductant is selected from formate, glucose, ethanol, ¾ _{, *} ¾ or mixtures thereof. Still more preferably, the reductant is ¾ or ¾ ₂ or mixtures thereof. Those skilled in the art can readily determine the most suitable reductant for a given application. For example, when high purity of the labelled cofactor or reduced reaction product is prioritised, the reductant is often preferably ¾. When reduced costs or high throughput is prioritised, the reductant is often preferably ¾. Most usually it is preferred that the reductant is ¾.

When the reductant is ¾ or *¾, the second polypeptide and/or the synthetic organic, inorganic or metallic oxidation catalyst is preferably selected or modified to catalyze ¾ or *¾ oxidation close to the thermodynamic potential E° of the 2EF/H ₂ couple

(“ E° (2EF/H ₂ )”) under the experimental conditions. (Those skilled in the art will appreciate that E° (2EF/H ₂ )

= -0.413 V at 25 °C, pH 7.0 and 1 bar ¾, and varies according to the Nemst equation). Preferably, the second polypeptide and/or the synthetic organic, inorganic or metallic oxidation catalyst is preferably selected or modified to catalyze ¾ or ^x ¾ oxidation at applied potentials of less than 100 mV more positive than E° (2HVH ₂ ); more preferably at applied potentials of less than 50 mV more positive than E° (2HVH ₂ ). Methods of determining the ability of a catalyst such as a second polypeptide or a synthetic organic, inorganic or metallic oxidation catalyst as defined herein to catalyze ¾ or *¾ oxidation close to E° (2HVH ₂ ) under the experimental conditions at issue are routine for those skilled in the art and are, for example, described in Vincent et al, J. Am. Chem. Soc. (2005) 127, 18179-18189.

When the electron source comprises a second polypeptide, the second polypeptide is preferably an oxidising enzyme or functional derivative or fragment thereof capable of oxidising a reductant to extract electrons, wherein the second polypeptide transfers electrons from the reductant to the first polypeptide via an electronically-conducting pathway. Those skilled in the art will appreciate that as used herein, an oxidising enzyme is an enzyme capable of oxidising a reductant to extract electrons and deliver those electrons to a suitable electronically-conducting pathway for transfer to the first polypeptide. As used herein, the term “oxidising enzyme” thus also includes enzymes such as oxidases and dehydrogenases.

When the electron source comprises a second polypeptide, the first polypeptide and the second polypeptide may constitute component parts of a modular, multidomain or multicomponent protein or protein complex. This is shown schematically in Figure 4.

When the first polypeptide and the second polypeptide constitute component parts of a modular, multidomain or multicomponent protein or protein complex, the first and second polypeptide are preferably either native partners or genetically fused redox partners. More preferably, the first and second polypeptide are native partners. As those skilled in the art will appreciate, native partners are associated together in vivo and are typically attached via non-covalent means such as by non-specific interactions, hydrophobic interactions, hydrophilic interactions (including hydrogen bonds), ionic interactions, and Van der Waals forces. In some embodiments, however, when the electron source comprises a second polypeptide, the first polypeptide and the second polypeptide are not native partners; i.e. they do not occur together in nature as an enzyme complex and in the cellular environment electrons are not transferred from the second polypeptide to the first polypeptide. In such embodiments, it is preferable that the first polypeptide and the second polypeptide are selected from or derived from different bacterial species or from different bacterial genera, or the first polypeptide and the second polypeptide are selected from or derived from the same bacterial genus or species, but from different enzymes within the said same bacterial genus or species.

When the first polypeptide and the second polypeptide constitute component parts of a modular, multidomain or multicomponent protein or protein complex, the electron-conducting pathway from the first polypeptide to the second polypeptide can comprise any suitable means. Preferably, the electron transfer pathway comprises metal centres such as metal atoms (e.g. in heme centres) or metal clusters, preferably iron-sulphur- containing clusters [FeS]-clusters. As those skilled in the art will appreciate, [FeS]-clusters include [3Fe4S] and [4Fe4S] clusters.

Preferably, when the electron source comprises a second polypeptide, the second polypeptide is selected or modified to oxidise ]¾ or *¾ (wherein x = 2 or 3) under the conditions of the method. More preferably the second polypeptide is a hydrogenase enzyme or a functional derivative or fragment thereof. Any suitable hydrogenase can be used. Preferably, the hydrogenase comprises an active site comprising iron atoms (as in the [FeFe]- hydrogenases) or both nickel and iron atoms (as in the [NiFe]- and [NiFeSe]- hydrogenases).

Preferably, when the electron source comprises a second polypeptide which is a hydrogenase, the hydrogenase is selected or modified to be oxygen tolerant. Oxygen tolerant hydrogenases are capable of oxidising ]¾ or ¾ in the presence of oxygen, such as in the presence of at least 0.01 % O2, preferably at least 0.1 % O2, more preferably at least 1% O2, such as at least 5% O2, e.g. at least 10% O2 such as at least 20% O2 or more whilst retaining at least 1%, preferably at least 5%, such as at least 10%, preferably at least 20%, more preferably at least 50% such as at least 80% e.g. at least 90% preferably at least 95% e.g. at least 99% of their ¾- or TE-oxidation activity under anaerobic conditions. Various oxygen-tolerant hydrogenases are known to those skilled in the art.

Preferably, when the electron source comprises a second polypeptide which is a hydrogenase, the hydrogenase comprises or consists of:

i) the amino acid sequence of Ralstonia eutropha soluble hydrogenase moiety (SEQ ID NOs: 30 and/or 31) or an amino acid sequence having at least 60% homology therewith; ii) the amino acid sequence of Ralstonia eutropha membrane-bound hydrogenase moiety (SEQ ID NOs: 32 and/or 33 and/or 34) or an amino acid sequence having at least 60% homology therewith;

iii) the amino acid sequence of Ralstonia eutropha regulatory hydrogenase moiety (SEQ ID NOs:

35 and/or 36) or an amino acid sequence having at least 60% homology therewith; iv) the amino acid sequence of Escherichia coli hydrogenase 1 (SEQ ID NOs:37 and/or 38) or an amino acid sequence having at least 60% homology therewith;

v) the amino acid sequence of Escherichia coli hydrogenase 2 (SEQ ID NOs:39 and/or 40) or an amino acid sequence having at least 60% homology therewith;

vi) the amino acid sequence of Aquifex aeolicus hydrogenase 1 (SEQ ID NO:41 and/or 42) or an amino acid sequence having at least 60% homology therewith;

vii) the amino acid sequence of Hydrogenovibrio marinus hydrogenase (SEQ ID NOs: 43 and/or 44) or an amino acid sequence having at least 60% homology therewith;

viii) the amino acid sequence of Thiocapsa roseopersicina hydrogenase (SEQ ID NOs: 45 and 46) or an amino acid sequence having at least 60% homology therewith;

ix) the amino acid sequence of Alteromonas macleodii hydrogenase (SEQ ID NOs: 47 and/or 48) or an amino acid sequence having at least 60% homology therewith;

x) the amino acid sequence of Rhodococcus opacus soluble hydrogenase moiety (SEQ ID NOs: 49 and/or 50) or an amino acid sequence having at least 60% homology therewith;

xi) the amino acid sequence of Allochromatium vinosum membrane bound hydrogenase (SEQ ID NOs: 51 and/ or 52) or an amino acid sequence having at least 60% homology therewith; xii) the amino acid sequence of Desulfovibrio fructosovorans membrane bound hydrogenase (SEQ ID NOs: 53 and/ or 54) or an amino acid sequence having at least 60% homology therewith; xiii) the amino acid sequence of Clostridium pasteurianum iron-iron hydrogenase (SEQ ID NOs: 55) or an amino acid sequence having at least 60% homology therewith;

xiv) the amino acid sequence of Clostridium acetobutylicum iron-iron hydrogenase (SEQ ID NOs:

56) or an amino acid sequence having at least 60% homology therewith;

xv) the amino acid sequence of Chlamydomonas reinhardtii iron-iron hydrogenase (SEQ ID NOs:

57) or an amino acid sequence having at least 60% homology therewith;

xvi) the amino acid sequence of Desulfomicrobium baculatum nickel-iron selenium hydrogenase (SEQ ID NOs: 58 and/ or 59) or an amino acid sequence having at least 60% homology therewith;

xvii) the amino acid sequence of Hydrogenophilus thermoluteolus soluble hydrogenase moiety (SEQ ID NOs: 60 and/or 61) or an amino acid sequence having at least 60% homology therewith; xviii) the amino acid sequence of Desulfovibrio vulgaris Nickel Iron hydrogenase (pdb 1H2A) (SEQ ID NOs: 62 and/ or 63) or an amino acid sequence having at least 60% homology therewith; xix) the amino acid sequence of Desulfovibrio gigas Periplasmic [NiFe] hydrogenase (SEQ ID NOs:

64 and/or 65) or an amino acid sequence having at least 60% homology therewith;

xx) the amino acid sequence of Salmonella enterica serovar Typhimurium LT2 nickel-iron

hydrogenase 5 (SEQ ID NO: 66 and/or 67) or an amino acid sequence having at least 60% homology therewith.

xxi) the amino acid sequence of Pyrococcus furiosus soluble alpha subunit (SEQ ID NOs: 68) or an amino acid sequence having at least 60% homology therewith; or a functional fragment, derivative or variant thereof.

When the electron source comprises a second polypeptide which is a hydrogenase, the hydrogenase may optionally not comprise a FMN and/or a FAD prosthetic group. Without being bound by theory, it is believed that hydrogenases lacking such groups typically have increased stability compared to hydrogenases comprising such prosthetic groups. Examples of hydrogenases lacking a FMN prosthetic group include Ralstonia eutropha membrane-bound hydrogenase (SEQ ID NOs: 32-34), Ralstonia eutropha regulatory hydrogenase (SEQ ID NOs:35-36), Escherichia coli hydrogenase 1 (SEQ ID NOs:37-38), Escherichia coli hydrogenase 2 (SEQ ID NOs:39-40), Aquifex aeolicus hydrogenase 1 (SEQ ID NOs:41-42),

Hydrogenovibrio marinus membrane-bound hydrogenase (SEQ ID NOs: 43-44), Desulfovibrio vulgaris Nickel Iron hydrogenase (SEQ ID NOs: 62-63) and Desulfovibrio gigas Periplasmic [NiFe] hydrogenase (SEQ ID NOs: 64-65). Such hydrogenases are particularly suitable when the first polypeptide and the second polypeptide constitute component parts of a modular, multidomain or multicomponent protein or protein complex.

Preferably, when the electron source comprises a second polypeptide which is a hydrogenase, the hydrogenase is selected from Escherichia coli hydrogenase 1 (SEQ ID NOs: 37,38), Escherichia coli hydrogenase 2 (SEQ ID NOs:39,40), Ralstonia eutropha soluble hydrogenase (HoxHY, SEQ ID NOs:

30,31), Hydrogenophilus thermoluteolus hydrogenase (SEQ ID NOs: 60,61), Desulfovibrio gigas hydrogenase (SEQ ID NO: 64,65), Desulfovibrio fructosovorans hydrogenase (SEQ ID NO: 53,54) and Desulfovibrio vulgaris (SEQ ID NO: 62,63), or an amino acid sequence having at least 60% homology therewith. Most preferably, the second polypeptide is Escherichia coli hydrogenase 1 (SEQ ID NOs: 37,38), Escherichia coli hydrogenase 2 (SEQ ID NOs: 39,40) or Ralstonia eutropha soluble hydrogenase (HoxHY, SEQ ID NOs: 30,31).

In other circumstances where it is preferable that the reductant is not ¾ or *¾, the second polypeptide may be preferably selected or modified to oxidise formate, glucose or an alcohol under the conditions of the method. When the reductant is glucose, the second polypeptide is preferably a glucose oxidase enzyme such as glucose dehydrogenase from Acinetobacter calcoaceticus (SEQ ID NO: 76), or Myriococcum thermophilum cellobiose dehydrogenase (SEQ ID NO: 75), or cellobiose dehydrogenase from Phanerochaete chrysosporium (SEQ ID NO: 73 and/or 74)) or an amino acid sequence having at least 60% homology therewith. When the reductant is an alcohol such as ethanol, the second polypeptide is preferably an alcohol dehydrogenase enzyme such as the PQQ- and heme-dependent ethanol dehydrogenase from Comamonas testosteroni (SEQ ID NO: 72). When the reductant is formate, the second polypeptide is preferably a formate dehydrogenase enzyme, more preferably the molybdenum-containing formate dehydrogenase H from Escherichia coli (EcFDH-H) (SEQ ID NO: 71) , or an amino acid sequence having at least 60% homology therewith; or the tungsten-containing formate dehydrogenase 1 from Desulfovibrio gigas (SEQ ID NO: 77 and/or 78) or an amino acid sequence having at least 60% homology therewith. Most preferably, when the reductant is formate, the second polypeptide is the molybdenum-containing formate dehydrogenase H from Escherichia coli (EcFDH-H) (SEQ ID NO: 71).

Preferably, when the second polypeptide comprises or consists of one or more amino acid sequences having at least 60% homology with a specified sequence, each amino acid sequence independently has at least 70%, such as at least 80%, more preferably at least 90%, e.g. at least 95%, preferably at least 97%, such as at least 98%, preferably at least 99% homology with the specified sequence. More preferably, each amino acid sequence independently has at least 70%, such as at least 80%, more preferably at least 90%, e.g. at least 95%, preferably at least 97%, such as at least 98%, preferably at least 99% identity with the specified sequence. For avoidance of doubt, if the second polypeptide comprises two or more amino acid sequences, the percentage homology of each of the two or more sequences with respect to their respective specified sequences can be the same or different. Percentage homology and/or percentage identity are each preferably determined across the length of the specified reference sequence.

As described herein the first polypeptide and/or the second polypeptide (if present) may be a functional fragment, derivative or variant of an enzyme or amino acid sequence. As those skilled in the art will appreciate, fragments of amino acid sequences include deletion variants of such sequences wherein one or more, such as at least 1, 2, 5, 10, 20, 50 or 100 amino acids are deleted. Deletion may occur at the C- terminus or N-terminus of the native sequence or within the native sequence. Typically, deletion of one or more amino acids does not influence the residues immediately surrounding the active site of an enzyme. Derivatives of amino acid sequences include post-translationally modified sequences including sequences which are modified in vivo or ex vivo. Many different protein modifications are known to those skilled in the art and include modifications to introduce new functionalities to amino acid residues, modifications to protect reactive amino acid residues or modifications to couple amino acid residues to chemical moieties such as reactive functional groups on linkers or substrates (surfaces) for attachment to such amino acid residues.

Derivatives of amino acid sequences include addition variants of such sequences wherein one or more, such as at least 1, 2, 5, 10, 20, 50 or 100 amino acids are added or introduced into the native sequence. Addition may occur at the C- terminus or N-terminus of the native sequence or within the native sequence. Typically, addition of one or more amino acids does not influence the residues immediately surrounding the active site of an enzyme.

Variants of amino acid sequences include sequences wherein one or more amino acid such as at least 1, 2, 5, 10, 20, 50 or 100 amino acid residues in the native sequence are exchanged for one or more non-native residues. Such variants can thus comprise point mutations or can be more profound e.g. native chemical ligation can be used to splice non-native amino acid sequences into partial native sequences to produce variants of native enzymes. Variants of amino acid sequences include sequences carrying naturally occurring amino acids and/or unnatural amino acids. Variants, derivatives and functional fragments of the aforementioned amino acid sequences retain at least some of the activity/ functionality of the native/ wild- type sequence. Preferably, variants, derivatives and functional fragments of the aforementioned sequences have increased/ improved activity/ functionality when compared to the native/ wild-type sequence.

When the electron source comprises a synthetic (i.e. non-biological) organic, inorganic or metallic oxidation catalyst, the catalyst is any synthetic organic, inorganic or metallic oxidation catalyst capable of oxidising a reductant to extract electrons. As used herein, a synthetic oxidation catalyst includes substances such as metals which occur naturally but which are non-biological. As used herein, enzymes are not synthetic catalysts. As explained below, exemplary synthetic catalysts include metals and metal-containing compounds such as metal oxides, metal hydroxides, and the like.

The synthetic (non-biological) catalyst oxidises the reductant to form an oxidised product. The electrons extracted from the reductant are transferred via an electron conducting pathway to the first polypeptide. The electrons are used by the first polypeptide to reduce the oxidised cofactor as described herein.

Preferably, when the electron source comprises a synthetic oxidation catalyst, the synthetic oxidation catalyst is selected or modified to oxidise ¾ or *¾ under the conditions of the method. Any suitable synthetic oxidation catalyst may be used. Many suitable H2/Ή2 oxidation catalysts are known to those skilled in the art and can be readily applied in the methods of the invention.

Preferably, when the electron source comprises a synthetic oxidation catalyst, the synthetic oxidation catalyst is capable of oxidising ¾ or ¾ in the presence of oxygen, such as in the presence of at least 0.01 % O2, preferably at least 0.1 % O2, more preferably at least 1% O2, such as at least 5% O2, e.g. at least 10% O2 such as at least 20% O2 or more whilst retaining at least 1%, preferably at least 5%, such as at least 10%, preferably at least 20%, more preferably at least 50% such as at least 80% e.g. at least 90% preferably at least 95% e.g. at least 99% of its ¾- or TL-oxidation activity under anaerobic conditions.

Preferably, the oxidation catalyst is a metal or metal-containing catalyst. Preferably, the oxidation catalyst comprises platinum, palladium, iridium, nickel, rhodium and/or ruthenium. More preferably, the oxidation catalyst comprises platinum. Many suitable metallic oxidation catalysts are known to those skilled in the art and can be readily applied in the methods of the invention. When the electron source comprises a non- metallic synthetic catalyst, any suitable non-metallic synthetic oxidation catalyst may be used. Preferable non-metallic synthetic oxidation catalysts include frustrated Lewis pair catalysts. Many such catalysts are known to those skilled in the art and can be readily applied in the methods of the invention.

In the methods of the invention, the electron source and the first polypeptide are preferably each in electronic contact with an electronically conducting support. More preferably, the electron source and the first polypeptide are each in electronic contact with the same electronically conducting support such that electrons flow from the electron source via the electronically conducting support to the first polypeptide.

Alternatively, the electron source may be in electronic contact with an electronically conducting first support and the first polypeptide in electronic contact with an electronically conducting second support; and the first support in electronic contact with the second support, such that electrons flow from the electron source to the electronically conducting first support, from the electronically conducting first support to the electronically conducting second support via the electronic contact between the first and second supports, and from the electronically conducting second support to the first polypeptide.

When the electron source and/or the first polypeptide are in electronic contact with a support, any suitable means of contact can be used. Preferably, the electron source and/or the first polypeptide are immobilized on the respective support(s). Any suitable means of contact can be used providing the electron source and/or the first polypeptide are immobilized in electronic contact with the support. As used herein, the term “immobilized” embraces adsorption, entrapment and/or cross-linkage between the support and the electron source or polypeptide. Adsorption embraces non-covalent interactions including electrostatic interactions, hydrophobic interactions, and the like. A charged adsorption enhancer such as polymyxin B sulphate can be used to enhance adsorption. Entrapment embraces containment of the electron source and/or the first polypeptide onto the surface of the support, e.g. within a polymeric film or in a hydrogel. Cross-linkage embraces covalent attachment, either directly between the electron source and/or the first polypeptide (e.g. via amide coupling, such as via EDC/NHS and/or other coupling agents routine to those skilled in the art) or using one or more covalent cross-linkers such as thiol-terminated linkers or crosslinking reagents.

Immobilization means comprising or consisting of adsorption are preferred. Combination of some or all of the above mentioned immobilization means may be used.

Preferably, the or each support independently comprises a material comprising carbon, a metal or metal alloy, a metal oxide (include mixed metal oxides), a metal hydroxide (including layered double hydroxides), a metal chalcogenide, a semi-conducting material (including silicates, germanium compounds and gallium compounds such as silicon carbide, doped silicon and/or doped germanium) or an electronically-conductive polymer; or mixtures thereof. As those skilled in the art will appreciated, suitable support materials can include mixtures of materials described herein, such as mixtures of metal oxides or mixed metal oxides. Any suitable support material can be used.

More preferably, the or each support material independently comprises:

i) carbon; and/or

ii) a metal or metal alloy selected from gold, silver, tungsten, iridium, platinum, palladium, copper, titanium, brass, and steel; and/or

iii) a material selected from titanium oxide, indium oxide, tin oxide and indium tin oxide. Still more preferably, the or each support material comprises a carbon material. Still more preferably, the or each support material independently comprises a carbon material comprising graphite, carbon nanotube(s), carbon black, activated carbon, carbon nanopowder, vitreous carbon, carbon fibre(s), carbon cloth, carbon felt, carbon paper, graphene, highly oriented pyrolytic graphite, pyrolytic graphite, or doped diamond. Most preferably, the or each support material independently comprises a carbon material comprising graphite (or highly oriented pyrolytic graphite or pyrolytic graphite) or carbon black; most preferably carbon black.

Preferably, the or each support is an electronically conducting particle. Preferred electronically conducting particles comprise materials described herein. Preferably, when the or each support comprise particles, the particles have a particle size of from about 1 nm to about 100 pm, such as from about 10 nm to about 10 pm e.g. from about 100 nm to about 1 pm. Methods of determining particle size are routine in the art and include, for example, dynamic light scattering. Suitable electronically conducting particles for use in the methods of the invention include conductive carbon black particles such as“Black Pearls 2000” particles available from Cabot corp (Boston, Mass., USA).

When the electron source comprises an electrode connected to an electrode controller, any suitable electrode material can be used. Preferred electrode materials comprise carbon, a metal or metal alloy, a metal oxide (include mixed metal oxides), a metal hydroxide (including layered double hydroxides), a metal chalcogenide, or an electronically-conductive polymer; or mixtures thereof. Suitable electrode materials can include mixtures of materials described herein, such as mixtures of metal oxides or mixed metal oxides.

Preferred electrode materials comprise:

i) carbon; and/or

ii) a metal or metal alloy selected from gold, silver, tungsten, iridium, platinum, palladium, copper, titanium, brass, and steel; and/or

iii) a material selected from titanium oxide, indium oxide, tin oxide and indium tin oxide.

More preferred electrode materials comprise a carbon material. Still more preferred electrode materials comprise a carbon material comprising graphite, carbon nanotube(s), carbon black, activated carbon, carbon nanopowder, vitreous carbon, carbon fibre(s), carbon cloth, carbon felt, carbon paper, graphene, highly oriented pyrolytic graphite, pyrolytic graphite, or doped diamond (e.g. boron-doped diamond). Most preferred electrode materials comprises carbon materials comprising graphite (or highly oriented pyrolytic graphite or pyrolytic graphite).

Preferably, in the methods of the invention, the first polypeptide and/or the electron source are provided in a form which can be easily removed from the reaction mixture. Preferably, the first polypeptide and the electron source comprise a heterogeneous system with the composition comprising Ή ⁺ ions. For example, the composition comprising Ή ⁺ ions is preferably a liquid and the first polypeptide and the electron source are in electronic contact with one or more electronically conducting support(s) which can be removed from the composition by sedimentation, filtration, centrifugation, or the like. For example, the first polypeptide and the electron source may be immobilized onto carbon materials as defined herein (e.g. carbon powder, carbon nanotubes, carbon black, carbon felt, activated carbon, or the like), and the carbon material(s) can be removed from the composition by sedimentation, filtration, centrifugation, etc. Many such methods are known to those skilled in the art, e.g. filtration can be achieved using a simple filter paper to remove solid components from a liquid composition; or a mixed solid/liquid composition can be allowed to settle and the liquid then decanted from the settled solids.

In the methods of the invention, electrons are transferred from the electron source to the first polypeptide. Preferably, electrons are directly transferred from the electron source to the first polypeptide along an electronically conducting pathway. Alternatively, electron transfer along the electronically-conducting pathway can be mediated by one or more electron mediators, as shown schematically in Figure 5. Suitable mediators include methyl viologen, benzyl viologen, methylene blue, flavin mononucleotide and flavin adenine dinucleotide.

In the methods of the invention, an electronically conducting pathway can be formed e.g. when the first polypeptide and the electron source are localised on the same electronically conducting supports. In another embodiment, the first polypeptide and the electron source can be localised or comprise or consist of different electronically conducting supports. In such cases the electronically-conducting pathway may comprise a linker such as a wire between the supports. The linker may be a molecular linker such as conductive polymeric strand or may be a metallic linker such as a metallic wire.

In the methods of the invention, the cofactor is preferably initially added to or present in an aqueous solution at a concentration of 1 mM to 1 M, such as from 5 mM to 800 mM, e.g. from 10 mM to 600 mM such as from 25 mM to 400 mM e.g. from 50 mM to 200 mM such as from 100 mM to about 100 mM e.g. from about 250 mM to about 10 mM such as from about 500 mM to about 1 mM.

The methods of the invention are typically conducted under a gas atmosphere; i.e. in the presence of gas (for example in the headspace of a reactor). Preferably, the gas atmosphere comprises an inert gas and/or hydrogen (Fh and/or ¾) optionally in the presence of Cfr. Preferred inert gases include nitrogen, argon, helium, neon, krypton, xenon, radon and sulfur hexafluoride (SFe) and mixtures thereof, more preferably nitrogen and/or argon, most preferably nitrogen. When the gas atmosphere comprises hydrogen (Fh or Ή2), the hydrogen is preferably present at a concentration of 1-100%, with the remaining gas comprising an inert gas as defined herein and/or (¾. Preferred gas atmospheres include from 80-100% Fh with the remaining gas comprising one or more inert gases; and from 0-20% Fh with the remaining gas comprising one or more inert gases and/or O2 (such as from 1-4% Fh in air). The gas atmosphere may optionally also include non-inert gases such as ammonia, carbon dioxide and hydrogen sulphide. Preferably, however, the gas atmosphere is free of ammonia, carbon dioxide and hydrogen sulphide.

The methods of the invention are typically conducted in an aqueous composition which may optionally comprise e.g. buffer salts. For some applications buffers are not required and the methods of the invention can be conducted without any buffering agents. Preferred buffer salts which can be used in the methods of the invention include Tris; phosphate; citric acid / Na2HP04; citric acid / sodium citrate; sodium acetate / acetic acid; Na2HP04 / NaEhPCri; imidazole (glyoxaline) / HC1; sodium carbonate / sodium bicarbonate; ammonium carbonate / ammonium bicarbonate; MES; Bis-Tris; ADA; aces; PIPES; MOPSO; Bis-Tris Propane; BES; MOPS; TES; HEPES; DIPSO; MOBS; TAPSO; Trizma; HEPPSO; POPSO; TEA; EPPS; Tricine; Gly-Gly; Bicine; HEPBS; TAPS; AMPD; TABS; AMPSO; CHES; CAPSO; AMP; CAPS and CABS. Selection of appropriate buffers for a desired pH is routine to those skilled in the art, and guidance is available at e.g. http://www.sigmaaldrich.com/life-science/core-bioreagents/bi ological-buffers/leaming- center/buffer-reference-center.html. Buffer salts used can be Ή-labelled, for example by exchanging labile protons for Ή ⁺ ions by dissolving the salt in an Ή-labelled solvent and subsequent solvent removal. Buffer salts are preferably used at concentrations of from 1 mM to 1 M, preferably from 10 mM to 100 mM such as about 50 mM in solution. Most preferred buffers for use in methods of the invention include 50 mM Tris- HC1, r(Ή) 8.0.

The methods of the invention are typically conducted in an aqueous composition. However, non-aqueous components can optionally be used instead or as well as water in the compositions used in the methods of the invention. For example, the compositions comprising Ή ⁺ ions may optionally comprise one or more organic solvents (e.g. alcohols) or one or more ionic liquids.

The methods of the invention can be used to make an oxidised labelled cofactor from a reduced labelled cofactor. Such methods involve the production of a singularly or doubly Ή-labelled reduced cofactor using methods of the invention as described herein and then removal of the non -required ¾ or Ή using an appropriate NADH-dependent enzyme to yield the oxidised labelled cofactor. This method is illustrated schematically in Figure 6. Suitable NADH-dependent enzymes for use in such methods include those enzymes used to produce reduced labelled reaction products as described herein. Preferably, the enzymes used in this step can selectively remove either the ( R ) or ( S ) Ή atom. For example, an ( R )- selective or ( S )- selective NADH- or NADPH-dependent oxidoreductase, such as an (K)-selective or (5)-selective alcohol dehydrogenase, may be used to provide the labelled oxidised cofactor.

For example, the method of the invention can be used to label an unlabelled cofactor to produce 4S- labelled reduced cofactor e.g. (45- ^x H)-NADH. Selective oxidation with an S-selective oxidoreductase, such as an ( S )- selective alcohol dehydrogenase, leaves a labelled oxidised cofactor, e.g. (4- ^x H)-NAD ⁺ . Further reaction of the labelled NAD ⁺ according to the methods of the invention can lead to a doubly Ή-labelled reduced cofactor at the 4-position.

When the methods of the invention comprise producing a reduced labelled reaction product comprising one or more Ή atom, the at least one enzyme that is an NADH-dependent oxidoreductase or an NADPH- dependent oxidoreductase or a functional derivative or fragment thereof is preferably at least one of an NAD(P)H-dependent alcohol dehydrogenase, an NAD(P)H-dependent ene reductase, an NAD(P)H- dependent imine reductase or an NAD(P)H-dependent amino-acid dehydrogenase. Other suitable NADH- dependent oxidoreductase or NADPH-dependent oxidoreductase enzymes include dehydrogenase, reductase, oxidase, synthase, transhydrogenase, dioxygenase and/or ene reductase enzymes. More preferably, the NADH-dependent oxidoreductase or NADPH-dependent oxidoreductase is at least one of an alcohol dehydrogenase or an amino acid dehydrogenase. As those skilled in the art will appreciate, any suitable NAD(P)H-dependent enzyme can be used, and the enzyme can be modified or selected to be specific for the desired reduction reaction. Variants, derivatives and functional fragments of the aforementioned oxidoreductases are also embraced by the present invention. Variants, derivatives and functional fragments of the aforementioned oxidoreductases retain at least some of the activity/ functionality of the native/ wild- type enzyme. Preferably, variants, derivatives and functional fragments of the aforementioned

oxidoreductases have increased/ improved activity/ functionality when compared to the native/ wild-type enzyme.

When the methods of the invention comprise producing a reduced labelled reaction product comprising one or more Ή atom, the at least one enzyme that is an NADH-dependent oxidoreductase or an NADPH- dependent oxidoreductase or a functional derivative or fragment thereof is preferably immobilised onto a support as defined herein. More preferably, the at least one enzyme that is an NADH-dependent oxidoreductase or an NADPH-dependent oxidoreductase or a functional derivative or fragment thereof is immobilised onto the same support as the first polypeptide and/or the electron source. Most preferably, the at least one enzyme that is an NADH-dependent oxidoreductase or an NADPH-dependent oxidoreductase or a functional derivative or fragment thereof is immobilised onto the same support as the first polypeptide and the electron source, as such configurations allow facile purification of the product by sedimentation, filtration, centrifugation, or the like as described herein.

The methods of the invention can be used to produce a variety of reduced labelled reaction products including alcohols, e.g. using alcohol dehydrogenases. For example, ketones, aldehydes, carboxylic acids and amino acids can be reduced to form labelled alcohols. Similarly imines can be reduced to form labelled amines, e.g. using imine reductases. Olefins (alkenes) can be reduced to alkane groups, e.g. using ene reductases. Labelled amines and amino acids can also be produced by reductive amination of ketones, e.g. using amine dehydrogenases or amino acid dehydrogenases. Accordingly, in preferred embodiments of the methods of the invention,

the composition comprising Ή ⁺ ions comprises ² ]¾0 or ³ ]¾0; and

the oxidised cofactor is NAD ⁺ , NADP ⁺ , or a labelled version of NAD ⁺ or NADP ⁺ comprising at least one Ή atom, wherein the Ή atom is at the 4- position of the nicotinamide ring.

In more preferred embodiments of the methods of the invention,

the composition comprising Ή ⁺ ions comprises ² ]¾0 or ³ ]¾0;

the oxidised cofactor is NAD ⁺ , NADP ⁺ , or a labelled version of NAD ⁺ or NADP ⁺ comprising at least one Ή atom, wherein the Ή atom is at the 4- position of the nicotinamide ring

the first polypeptide is one or more of the amino acid sequences of any one of SEQ ID NOs 1 to 29 or 69 to 70, or an amino acid sequence having at least 60% homology (such as at least 70%, at least 80%, at least 90% or at least 95% homology) therewith;

the electron source is a second polypeptide or a synthetic organic, inorganic or metallic oxidation catalyst or an electrode connected to an electrode controller; wherein optionally:

o the second polypeptide is one or more of the amino acid sequences of any one of SEQ ID NOs 30 to 68, or an amino acid sequence having at least 60% homology (such as at least 70%, at least 80%, at least 90% or at least 95% homology) therewith; and/or o the synthetic oxidation catalyst comprises platinum, palladium, iridium, nickel, rhodium and/or ruthenium; or is frustrated Lewis pair catalyst; and/or

o the reductant is ¾ or *¾ wherein x = 2 or 3; and/or

o the electrode material comprises:

carbon; and/or

a metal or metal alloy selected from gold, silver, tungsten, iridium, platinum, palladium, copper, titanium, brass, and steel; and/or

a material selected from titanium oxide, indium oxide, tin oxide, indium tin oxide and

i) the electron source and the first polypeptide each comprise or are in electronic contact with an electronically conducting support; wherein optionally the support material comprises: carbon; and/or

a metal or metal alloy selected from gold, silver, tungsten, iridium, platinum, palladium, copper, titanium, brass, and steel; and/or

a material selected from titanium oxide, indium oxide, tin oxide, indium tin oxide; or

ii) the first polypeptide and the second polypeptide constitute component parts of a modular, multidomain or multicomponent protein or protein complex.

In still more preferred embodiments of the methods of the invention,

the composition comprising Ή ⁺ ions comprises ² ]¾0; the oxidised cofactor is NAD ⁺ or a labelled version of NAD ⁺ comprising at least one Ή atom, wherein the Ή atom is at the 4- position of the nicotinamide ring;

the first polypeptide is the HoxHYFU tetramer of Ralstonia eutropha (SEQ ID NOs: 1,2,30,31), or an amino acid sequence having at least 60% homology (such as at least 70%, at least 80%, at least 90% or at least 95% homology) therewith; wherein optionally the HoxH moiety is a non- functional variant comprising the point mutation I64A (SEQ ID NO: 69);

the electron source is a second polypeptide or a synthetic organic, inorganic or metallic oxidation catalyst, or an electrode connected to an electrode controller; wherein optionally:

o the second polypeptide is one or more of the amino acid sequences of any one of SEQ ID NOs 30-31, 37-40, 53-54 and/or 60-65, or an amino acid sequence having at least 80% homology (such as at least 90% or at least 95% homology) therewith; and/or o the synthetic oxidation catalyst comprises platinum; and

o the reductant is ¾ and/or

o the electrode material comprises carbon;

and

i) the electron source and the first polypeptide each comprise or are in electronic contact with the same electronically conducting support; wherein optionally the support material comprises carbon

or

ii) the first polypeptide and the second polypeptide constitute component parts of a modular, multidomain or multicomponent protein or protein complex.

The invention also provides a system for performing a method of the invention, the system comprising: i) a composition comprising (i) Ή ⁺ ions wherein x is 2 or 3 ; and (ii) an oxidised cofactor, wherein preferably the oxidised cofactor and/or the composition is as defined herein;

ii) an electron source, wherein preferably the electron source is as defined herein; and

iii) a first polypeptide which is an NADH: acceptor oxidoreductase or an NADPH: acceptor

oxidoreductase or a functional derivative or fragment thereof, wherein preferably the first polypeptide is as defined herein;

wherein the system is configured such that, in use, (a) electrons are transferred from the electron source to the first polypeptide and (b) Ή ⁺ ions and the oxidised cofactor are contacted with the first polypeptide so as to reduce the oxidised cofactor to form a reduced labelled cofactor comprising one or more Ή atoms.

The following Examples illustrate the invention. They do not, however, limit the invention in any way. In this regard, it is important to understand that the particular assays used in the Examples section are designed only to provide an indication of the efficacy of the method of the invention. There are many assays available to determine reaction efficiency and labelling success, and a negative result in any one particular assay is therefore not determinative.

Examples Protein expression

Methods for expression of proteins in cellular (e.g. microbial) expression systems are well known and routine to those skilled in the art. For example, the first polypeptide and the second polypeptide (if present) can be independently isolated from their host organisms using routine purification methods. For example, host cells can be grown in a suitable medium. Lysing of cells allows internal components of the cells to be accessed. Membrane proteins can be solubilised with detergents such as Triton X (e.g. Triton X-l 14, (1,1,3,3- Tetramethylbutyl)phenyl-poly ethylene glycol, available from Sigma Aldrich). Soluble or solubilized proteins can be isolated and purified using standard chromatographic techniques such as size exclusion chromatography, ion exchange chromatography and hydrophobic interaction chromatography. Alternatively, the first polypeptide and the second polypeptide (if present) can be independently encoded in one or more nucleotide vector and subsequently expressed in an appropriate host cell (e.g. a microbial cell, such as E. coll). Purification tags such as a HIS (hexa-histidine) tag can be encoded (typically at the C- or N- terminal of the relevant polypeptide) and can be used to isolate the tagged protein using affinity chromatography for example using nickel- or cobalt-NTA chromatography. If desired, protease recognition sequences can be incorporated between the first and/or second polypeptide and the affinity purification tag to allow the tag to be removed post expression. Such techniques are routine to those skilled in the art and are described in, for example, Sambrook et al,“Molecular Cloning: A Laboratory Manual”, Cold Spring Harbor Laboratory Press.

Sequence Homology

Standard methods in the art may be used to determine homology. For example the UWGCG Package provides the BESTFIT program which can be used to calculate homology, for example used on its default settings (Devereux et al (1984) Nucleic Acids Research 12, p387-395). The PILEUP and BLAST algorithms can be used to calculate homology or line up sequences (such as identifying equivalent residues or corresponding sequences (typically on their default settings)), for example as described in Altschul S. F. (1993) J Mol Evol 36:290-300; Altschul, S.F et al (1990) J Mol Biol 215:403-10). Software for performing BLAST analyses is publicly available through the National Center for Biotechnology Information

(http://www.ncbi.nlm.nih.gov/). Similarity can be measured using pairwise identity or by applying a scoring matrix such as BLOSUM62 and converting to an equivalent identity. Since they represent functional rather than evolved changes, deliberately mutated positions would be masked when determining homology. Similarity may be determined more sensitively by the application of position-specific scoring matrices using, for example, PSIBLAST on a comprehensive database of protein sequences. A different scoring matrix could be used that reflect amino acid chemico-physical properties rather than frequency of substitution over evolutionary time scales (e.g. charge). Conservative substitutions replace amino acids with other amino acids of similar chemical structure, similar chemical properties or similar side-chain volume. The amino acids introduced may have similar polarity, hydrophilicity, hydrophobicity, basicity, acidity, neutrality or charge to the amino acids they replace. Alternatively, the conservative substitution may introduce another amino acid that is aromatic or aliphatic in the place of a pre-existing aromatic or aliphatic amino acid. Conservative amino acid changes are well-known in the art and may be selected in accordance with the properties of the 20 main amino acids as defined in Table A below. Where amino acids have similar polarity, this can also be determined by reference to the hydropathy scale for amino acid side chains in Table B.

Table A - Chemical properties of amino acids

Table B - Hydropathy scale

Side Chain Hydropathy

lie 4.5

Val 4.2

Leu 3.8

Phe 2.8

Cys 2.5

Met 1.9

Ala 1.8

Gly -0.4

Thr -0.7

Ser 0.8

Trp -0.9

Tyr -1.3

Pro 1.6

His -3.2

Glu -3.5

Gin -3.5

Asp -3.5

Asn -3.5

Lys -3.9

Arg -4.5

Preferably, sequence homology can be assessed in terms of sequence identity. Any of a variety of sequence alignment methods can be used to determine percent identity, including, without limitation, global methods, local methods and hybrid methods, such as, e.g., segment approach methods. Protocols to determine percent identity are routine procedures within the scope of those skilled in the art. Global methods align sequences from the beginning to the end of the molecule and determine the best alignment by adding up scores of individual residue pairs and by imposing gap penalties. Preferred methods include CLUSTAL W (Thompson et al., Nucleic Acids Research, 22(22) 4673-4680 (1994)) and iterative refinement (Gotoh, J. Mol. Biol. 264(4) 823-838 (1996)). Local methods align sequences by identifying one or more conserved motifs shared by all of the input sequences. Preferred methods include Match-box, (Depiereux and Feytmans, CABIOS 8(5) 501 -509 (1992)); Gibbs sampling, (Lawrence et al., Science 262(5131) 208-214 (1993)); and Align-M (Van Walle et al., Bioinformatics, 20(9) 1428-1435 (2004)). Thus, percent sequence identity is determined by conventional methods. See, for example, Altschul et al., Bull. Math. Bio. 48: 603-16, 1986 and Henikoff and Henikoff, Proc. Natl. Acad. Sci. USA 89: 10915-19, 1992. Briefly, two amino acid sequences are aligned to optimize the alignment scores using a gap opening penalty of 10, a gap extension penalty of 1 , and the "blosum 62" scoring matrix of Henikoff and Henikoff (ibid.) as shown below (amino acids are indicated by the standard one-letter codes). Alignment scores for determining sequence identity

A R N D C Q E G H I L K M F P S T W Y v

A 4

R -1 5

N -2 0 6

D -2 -2 1 6

C 0 -3 -3 -3 9

Q -1 1 0 0 -3 5

E -1 0 0 2 -4 2 5

G 0 -2 0 -1 -3 -2 -2 6

H -2 0 1 -1 -3 0 0 -2 8

I -1 -3 -3 -3 -1 -3 -3 -4 -3 4

L -1 -2 -3 -4 -1 -2 -3 -4 -3 2 4

K -1 2 0 -1 -3 1 1 -2 -1 -3 -2 5

M -1 -1 -2 -3 -1 0 -2 -3 -2 1 2 -1 5

F -2 -3 -3 -3 -2 -3 -3 -3 -1 0 0 -3 0 6

P -1 -2 -2 -1 -3 -1 -1 -2 -2 -3 -3 -1 -2 -4 7

S 1 -1 1 0 -1 0 0 0 -1 -2 -2 0 -1 -2 -1 4

T 0 -1 0 -1 -1 -1 -1 -2 -2 -1 -1 -1 -1 -2 -1 1 5

W -3 -3 -4 -4 -2 -2 -3 -2 -2 -3 -2 -3 -1 1 -4 -3 -2 11

Y -2 -2 -2 -3 -2 -1 -2 -3 2 -1 -1 -2 -1 3 -3 -2 -2 2 7

V 0 -3 -3 -3 -1 -2 -2 -3 -3 3 1 -2 1 -1 -2 -2 0 -3 -1 4

Percent identity is then calculated as:

100 x (T/L)

where

T = Total number of identical matches

L = Length of the longer sequence plus the number of gaps introduced into the longer sequence in order to align the two sequences

Materials and reagents

General reagents and buffer salts (Sigma Aldrich), NAD ⁺ and NADP ⁺ (Prozomix), Pt/C (nominally 20 wt.%, Alfa Aesar), and carbon black particles (Black Pearls 2000, BP2000, Cabot Corporation), were all used as received without further purification. All non-deuterated solutions were prepared with MilliQ water (Millipore, 18 M cm), and deuterated solutions with ² ¾0 (99.98 %, Sigma Aldrich). All solvents were deoxygenated by sparging with dry N2 for 60 minutes prior to use.

[ ² H5]-Tris. ² HCl was prepared by dissolving the required amount of Trizma® base in ² ¾0 and then evaporating to dryness. After repeating twice more, the pD (p ² H) of the Tris solution was adjusted to 8.0 by the addition of small aliquots of ² HC1 (3.0 M). To preserve the isotopic purity of the buffer solution, the sample was deoxygenated with N2 that had first been bubbled through sacrificial ² ]¾0. Comparison to the Tris peak (£ = 3.70 ppm) in the NMR spectrum indicated that the final % ² H2q was not below 99 mol.% (unless specifically diluted with ¾0). pD (p ² H) is measured as described in Covington et al. ( Anal Chem. (1968) 40 (4), 700-706). Enzyme purification and isolation

R. eutropha soluble hydrogenase (SH; SEQ ID NOs: 1,2,3,30,31) was prepared as described in Lauterbach et al, FEBSJ., 2013, 280, 3058-3068 and Lauterbach and Lenz, J. Am. Chem. Soc., 2013, 135, 17897-905. E. coli hydrogenase 1 (Hydl, SEQ ID NOs: 37-38) and E. coli hydrogenase 2 (Hyd2; SEQ ID NOs: 39-40) were prepared as described in Lukey et al, J. Biol. Chem., 2010, 285, 3928-3938. R. eutropha NAD ⁺ reductase (HoxHYFU, also referred to as NAD-R; SEQ ID NOs: 1,2,31,69) was prepared as described in Lauterbach and Lenz, J. Am. Chem. Soc., 2013, 135, 17897-17905. Commercial samples of alcohol dehydrogenases (ADH101 and ADH105, Johnson Matthey Catalysis and Chiral Technologies), ene-reductase (ENE107, Johnson Matthey Catalysis and Chiral Technologies), L-alanine dehydrogenase (Sigma) were all received in their lyophilised forms and used without modification. ADH101 (Johnson Matthey Catalysis and Chiral Technologies) is a (R)-selective (“pro-R”) ketone reductase (alcohol dehydrogenase). ADH105 (Johnson Matthey Catalysis and Chiral Technologies) is an (S) selective (“pro-S”) ketone reductase (alcohol dehydrogenase).

As discussed above, R. eutropha soluble hydrogenase (SH) comprises 4 subunits HoxHYFU, with HoxHY being related to ¾/H ⁺ cycling and HoxFU to NAD ⁺ /NADH. The HoxHY subunit is relatively unstable, but can be rendered obsolete by a single amino acid mutation (I64A) to a yield a more robust construct:

HoxHYFU. HoxHYFU can be considered to be a stabilised NAD ⁺ -reductase (diaphorase) suitable for coupling to various other external H2-oxidising systems, and is abbreviated to“NAD-R” for ease.

Catalyst syntheses

All catalysts were prepared in a glovebox under a protective N2 atmosphere (O2 < 0.1 ppm), and in deoxygenated Tris-HCl (100 mM, pH 8.0). When the reaction was to be carried out under deuterated conditions, the non-isotopically enriched catalyst solution was centrifuged (12 000 rpm, 5 mins), decanted, and the solid re-suspended in an equal volume of [ ² H5]-Tris. ² HCl (100 mM, pD 8.0).

Pt/C was prepared by sonication of a 20 mg/mL suspension for 5 x 15 minutes (with agitation of the solution in between). Suspensions of Pt/C were allowed to stand for between 15 minutes and 24 hours prior to use.

For Pt+NAD-R/C, an aliquot of NAD+ reductase (1.4 mg/mL) was added to an equal volume of the Pt/C suspension and allowed to stand at 4 °C for 60 minutes prior to centrifugation (12 000 rpm, 5 mins), removal of the liquid, and re-suspension in the deuterated or non-deuterated buffer.

For experiments utilising carbon black, a suspension of BP2000 (20 mg/mL) was sonicated in the same manner as Pt/C. Particles of H2ase+NAD-R/C were then prepared by pre-mixing aliquots of the enzymes, and then adding them to a defined volume of BP2000. The H2ase+NAD-R/C particles then stood at 4 ^° C for 60 minutes, prior to centrifugation (12 000 rpm, 5 mins), removal of the excess solution, and re-suspension in the deuterated or non-deuterated buffer. Enzyme-modified particles were then used immediately, or snap- frozen in liquid N2 and stored at -80 ^° C prior to use. Whilst no attempt was made to quantify the degree of enzyme immobilisation, a considerable reduction in the brown hue of the solutions indicated that it was very high. If an additional enzyme (namely the NADH-dependent oxidoreductases) was to be co-immobilised on to the particles, this was done using a very large excess, after the particles had already been coated with H2ase and NAD-R.

Reaction conditions

All reactions were set up in a glovebox under a protective N2 atmosphere (O2 < 0.1 ppm) and were conducted on a 500 pL scale in sealed 1.5 mL micro-centrifuge tubes (Eppendorf) punctured with a single hole in the lid (0 1.0 mm). Solid catalysts were typically added at a loading of 100 /ig(C)/mL and SH was added at 20 /iL/mL. In order to help dissolve organic compounds such as AcPh, 2.0 - 5.0 vol.% ( ² ¾)- dimethylsulphoxide was included in the reactions as required (with the deuterium label serving only to ease analysis, and playing no part in the reaction). The sealed tubes were then transferred to a Tinyclave pressure vessel (Buchi) and were charged with 2 bar partial pressures of ¾ or ² H2 as required. The vessel was laid horizontally and rocked back and forth at 15 rpm whilst the reactions took place. Alternatively, a modified shaker was used that enabled a steady flow of the selected hydrogen gas across the reaction headspace with simultaneous agitation.

Product analysis

Following depressurisation of the reaction vessel, the catalyst was separated from the reaction mixture by two rounds of centrifugations (10,000 ^x g, 5 mins) or by filtration through a nylon syringe filter (Gilson,

0.22 pm). The solutions were then subject to one or more of the following analyses: ¾ NMR spectroscopy, UV-Vis spectroscopy, high-performance liquid chromatography (HPLC), and gas chromatography (GC). The general methods for each of these techniques are described below:

'7/ NMR spectroscopy

Following removal of the catalyst particles by filtration and centrifugation, 350 - 450 pL of the sample solution was transferred to a Norell® SelectSeries™ 5 mm 400 MHz sample tube. A further 50 - 150 pL of ¾ ₂ 0 was added for field locking purposes and, when required, 0.5 mM of acetone or 1.0 mM of 4,4- dimethyl-4-silapentane-l -sulfonic acid (DSS) was also included to act as a reference. ¾ NMR spectroscopy was carried out on either a Bruker Avance III HD nanobay (400 MHz) or Bruker Avance III (500 MHz) instrument, with samples for direct comparison always being run on the same machine. Both machines were equipped with 5 mm z-gradient broadband multinuclear probes. Spectra were acquired according to the parameters in the Table below. Data were acquired using either the standard Bruker ¾ ID zg30 pulse program, or, for samples requiring solvent suppression, the noesygpprld program.

Machine Avance III - 400 Avance III - 500

Experiment ¾ ¾

RF pulse energy (MHz) 400.13 499.9

Temperature (K) 298 ± 2 298 ± 2

Number of scans 32 32

Pulse width (us) 14.0 10.3

Spectral width (Hz) 8000 8000

Acquisition time (s) 4.09 2.04

Relaxation delay (s) 1.00 2.00

In the first instance, the Bruker proc_ld or proc_ldakps processing algorithms were applied, followed by additional manual re-phasing where necessary. A multipoint baseline correction was also applied across the entirety of the spectral window and a line broadening corresponding to 0.3 Hz was applied to each spectrum to improve the S/N ratio. Signals were referenced against an internal acetone standard ( d = 2.22 ppm), DMSO ( 5 = 2.71), or the Tris peak ( d = 3.70 ppm), all of which were referenced originally to DSS ( d = 0.00 ppm).

The spectra of nicotinamide cofactors and their deuterated analogues were assigned according to well established literature arguments (see for example Figure 7; reproduced from Hirst et al., Biochemistry 2013, 52, 4048-4055). Comparison of the peak(s) between 2.64 - 2.84 ppm (corresponding to protons on the 4- position of the dihydronicotinamide ring) were used to discern the relative abundance of the various isotopologues of NADH in solution. Control experiments showed that, within experimental error, the isotopic constitution of the NMR solvent does not influence the interpretation of the isotopic constitution of the NADH. Values of > 95 % isotopic purity are quoted to reflect the limit of detection in the experimental setup used, and do not necessarily indicate that other isotopologues were generated.

HPLC

All HPLC was conducted on a Shimadzu UFLC LC-20AD prominence liquid chromatograph equipped with a dual wavelength UV-spectrophotometric detection. MilliQ water and HPLC grade solvents were used throughout. The following protocols were used depending on the nature of the analytes followed:

HPLC Method A

Description: Hydrophilic Interaction Liquid Chromatography (HILIC) for cofactor analysis Sample: Samples were first filtered through a nylon syringe filter (Gilson, 0.22 /on), and then centrifuged at 14, 000 rpm for 5 minutes to remove any smaller particulates. 50 vol.% MeCN was added to the samples, prior to an additional round of centrifugation and transfer to glass HPLC vials.

Column: SeQuant® ZIC®-HILIC, 5 pM particle size, 200 A pore size, 150 X 4.6 mm bed, equipped with a 20 X 2.1 mm guard

Buffer A: 90 vol.% MeCN (Honeywell, CHROMASOLV® 99.9%): 10 vol.% MilliQ, 20 mM ammonium acetate, pH 7.5

Buffer B: 100 vol.% MilliQ, 20 mM ammonium acetate, pH 7.5

Column temperature = 40 ^° C

Flow rate = 1 mL/min

Injection volume = 10 pL

Detection = 260 and 340 nm

Pump profile

Time (minutes) Solvent ratio (vol% A : vol% B)

0 ® 1 100 : 0

1 ® 31 100 : 0 ® 20 : 80 (linear gradient)

31 ® 33 20 : 80

33 ® 35 100 : 0

HPLC Method B

Description: Chiral HPLC for resolution of stereoisomers

Sample: Samples were extracted with a 2 ^c volume of heptane : 2-propanol (99: 1 vol/vol), and then centrifuged at 14, 000 rpm for 5 minutes before being transferred to glass vials for HPLC.

Column: Chiralpak IA column (15 cm x 4.6 mm, 5 pm particle size) equipped with a 20 x 2.1 mm guard column

Buffer: heptane : 2-propanol (99: 1 vol/vol)

Column temperature = 40 ^° C

Flow rate = 1 mL/min

Injection volume = 10 pL

Detection = 210 nm

Pump profile = isocratic over 15 minutes

GC

GC was carried out on a ThermoScientific Trace 1310 equipped with an autosampler. Sample: Samples were extracted with a 2 ^c volume of ethyl acetate, and then centrifuged at 14, 000 rpm for 5 minutes before being transferred to glass vials for GC.

Column: DB-1701 (agilent), 30 m length, 0.25 mm diameter, 0.25 /an (film thickness)

Carrier: He (CP grade), 0.5 mL minute (constant flow)

Detection: FID (¾ = 25 mL/min, air = 350 mL/min, makeup N2 = 40 mL/min)

Oven profile:

Time (minutes) Oven

0 2 Hold at 40°C

2 23 Ramp to 250 °C at 10 "C/min

23 33 Hold at 250 °C for 10 mins

UV-vis spectroscopy

Reactions which resulted in changes in the relatative concentration of NAD(P) ⁺ /NAD(P)H could be followed be UV-vis spectroscopy. Typically, solid particulates were removed from the solution by filtration or centrifugation (as described above) and the sample diluted in MilliQ (¾0) water so that the cofactors were in the range 0.1 - 0.2 mM. A background spectrum of pure MilliQ was subtracted from that acquired for the sample. Measurements were made in a quartz cuvette (path length 1 cm, Hellma) on a Cary 60 UV/Vis spectrophotometer (Agilent). The ratio of NAD ⁺ to NADH could then be determined by measuring the ratio of A26O nm · A340 nm·

Example 1

Examples 1A -1C demonstrate the method of the invention with the electron source being a second polypeptide and the first and second polypeptides not being component parts of an enzyme complex.

Example 1A

Carbon particles were modified with NAD ⁺ -reductase (NAD-R, i.e. R. eutropha soluble hydrogenase with an inactivated hydrogenase moiety, I64A, SEQ ID NOs: 1,2,31,69) as the first polypeptide and E. coli hydrogenase 2 (SEQ ID NOs: 39-40) as the second polypeptide, as described above. The NAD ⁺ -reductase and hydrogenase are not native redox partners in vivo. Enzymes were not exchanged into deuterated buffer. Enzymes were prepared following standard protocols. Carbon particles (Black Pearls 2000) were prepared by sonication for 90 minutes in [ ² H5]-Tris. ² HCl (100 mM, p ² H 8.0) at a concentration of 20 mg mL ¹ . A mixture of the hydrogenase and NAD ⁺ -reductase (each of a concentration of between 1 - 2 mg/mL) was added to an aliquot of carbon particles and left at 4 °C for 90 minutes. The particles were then centrifuged (12 000 rpm, 2 mins) and the supernatant removed and replaced with sufficient ² H5-Tris. ² HCl to give a concentration of 10 mg(C)/mL. Enzyme loading was determined as 3 - 5 /<g of each enzyme per 100 <g(C) (assuming enzymes were fully immobilised).

An aliquot containing 100 m% of enzyme modified particles was then added to 500 mE of [ ² Hs]-Tris. ² HCl (100 mM in ² ¾0, p ² H 8.0) containing 1.0 mM NAD ⁺ , which had been pre-saturated with ¾ gas. The reaction solution was subsequently sealed in a pressure vessel under 2 bar of ¾ and rocked at 15 rpm for 18 hours at 20 ^° C.

Production of reduced cofactor (NADH) was monitored by UV-Visible spectroscopy with the characteristic peak observed at 340 nm indicative of formation of the reduced cofactor. Confirmation of the isotopic composition of the NADH was made by ¾ NMR spectroscopy. The general procedures for these methods are described above.

UV-visible spectra (Figure 8A) demonstrated generation of reduced cofactor at a conversion of > 95 %.

¾ NMR spectroscopy (Figure 8B) of the final reaction solution showed generation of a product having a single singlet peak at a chemical shift of S = 2.77 ppm (expanded region shown in Figure 8C) confirming generation of deuterated cofactor. Comparison with literature spectra (Figure 7; reproduced from Hirst et al., Biochemistry 2013, 52, 4048-4055) confirmed that the produced product is [45- ² H]-NADH only. >95 % incorporation of ² H was observed. The observed >95% incorporation reflects the limit of detection in the experimental setup used, and does not indicate any generation of [4- ¹ H]-NADH.

The ¾ NMR spectra shown in Figure 8B were generated with the following parameters: 400 MHz, 128 scans, water suppression, LB = 0.3 Hz, ² ¾0 (p ² H 8.0), 298 K

Example IB

The reaction was conducted in a similar manner to that described in Example 1 A, but using E. coli hydrogenase 1 (SEQ ID NOs: 37-38) as the second polypeptide.

In brief, the following conditions were used: 100 <g(C) with 15 - 20 m% of immobilised hydrogenase (E. coli hydrogenase 1) and NAD ⁺ reductase (NAD-R, SEQ ID NOs: 1,2,31,69) was suspended in 500/<L

[ ² H5]-Tris. ² HCl (100 mM in ² ¾0, p ² H 8.0) containing 4 mM NAD ⁺ which had been pre-saturated with ¾ gas. The reaction solution was subsequently sealed in a pressure vessel under 2 bar of ¾ and rocked at 30 rpm for 16 hours at 20°C.

Product analysis as described in Example 1 A showed high conversion (> 95 %) to NADH, with high selectivity (> 95 %) for the [4S- ² H]-NADH isotopomer (see Figures 9A, 9B and 9C). The ¾ NMR spectra shown in Figures 9B and 9C were generated with the following parameters: 400 MHz,

8 scans, water suppression, LB = 0.3 Hz, ² H ₂ 0 (p ² H 8.0), 298 K

Example 1C

The reaction was conducted in a similar manner to that described in Example 1 A, but using E. coli hydrogenase 1 (SEQ ID NOs: 37-38) as the second polypeptide and HoxF NAD ⁺ reductase (SEQ ID NO: 1) as the first polypeptide.

In brief, the following conditions were used: 200 mg(C) with 40 m of immobilised hydrogenase and NAD ⁺ reductase was suspended in 800/<L [ ² Hs]-Tris. ² HCl (100 mM in ² H ₂ 0, p ² H 8.0) containing 3.5 mM NAD ⁺ which had been pre-saturated with ¾ gas. The reaction solution was subsequently sealed in a shaker plate under a steady stream of ¾ and shaken at 500 rpm for 16 hours at 20°C.

Product analysis as described in Example 1 A showed a conversion of around 60 % to NADH, with high selectivity (> 95 %) for the [45- ² H]-NADH isotopomer (see Figures 10A, 10B and 10C).

The ¾ NMR spectra shown in Figure 10B and 10C were generated with the following parameters: 500 MHz, 64 scans, LB = 0.3 Hz, ² H ₂ 0 (p ² H 8.0), 298 K.

Example 2

This Example demonstrates the method of the invention with the electron source being a second polypeptide and the first and second polypeptides being component parts of an enzyme complex.

R. eutropha soluble hydrogenase (SEQ ID NOs: 1,2,3,30,31) was placed in 500 mE [ ² H5]-Tris. ² HCl (100 mM in ² H ₂ 0, p ² H 8.0) containing 1 mM NAD ⁺ . The reaction solution was subsequently sealed in a pressure vessel under 2 bar of ¾ and rocked at 15 rpm for 15 hours at 20°C.

Product analysis as described in Example 1 A showed high conversion (> 95 %) to NADH, with high selectivity (> 95 %) for the [45- ² H]-NADH isotopomer (see Figures 11 A, 1 IB and 11C). The identity of the product ([4- ² H]-NADH as opposed to [4- ¹ H]-NADH) was confirmed by 'H-NMR spectroscopy. This experiment confirms that it is not necessary to use labelled reductant if operating in ² H ₂ 0.

The ¾ NMR spectra shown in Figure 1 IB and 11C were generated with the following parameters: 400 MHz, 32 scans, LB = 0.3 Hz, ² H ₂ 0 (p ² H 8.0), 298 K. Example 3

This Example demonstrates the method of the invention with the electron source being a carbon electrode.

R. eutropha soluble hydrogenase with inactive hydrogenase (NAD-R, SEQ ID NOs: 1,2,31,69) was immobilised on carbon particles (Black Pearls 2000) as described in Example 1 A. The carbon particles were then immobilised on a 3 mm diameter pyrolytic graphite edge rotating disk electrode (see Lauterbach et al, PLoS ONE; doi: 10.1371/joumal.pone.0025939). The enzyme-modified particles were deposited on the electrode and allowed to partially dry over ca 2 minutes before submersing into the electrochemical cell.

The modified electrode was placed in an electrochemical cell containing NAD ⁺ (10 mM) in 5 mL [ ² f¾]- Tris. ² HCl (100 mM in ² ¾0, p ² H 8.0) and rotated at 1000 rpm. The electrode was held at -0.75 V vs SCE (SCE = saturated calomel electrode; SCE = +0.248V vs SHE at 20 °C) for 16 hours. At this potential, no direct reduction of the cofactor at the electrode is observed.

Product analysis as described in Example 1 A showed a conversion of around 50 % to NADH, with high selectivity (> 95 %) for the [45- ² H]-NADH isotopomer (see Figures 12A, 12B and 12C).

The ¾ NMR spectra shown in Figure 12B and 12C were generated with the following parameters: 400 MHz, 256 scans, LB = 0.3 Hz, ² ¾0 (p ² H 8.0), 298 K, multipoint baseline correction.

Example 4

This Example demonstrates the method of the invention for the generation of labelled-NADPH, with the electron source being a second polypeptide and the first and second polypeptides not being component parts of an enzyme complex.

The reaction was conducted in a similar manner to that described in Example 1 A, but using E. coli hydrogenase 2 (SEQ ID NOs: 39-40) as the second polypeptide and HoxHYF ^E341A+D467S U (SEQ ID NOs: 2, 30,31,70) as the first polypeptide.

The following conditions were used: 100 mg(C) with 6 /<g of immobilised hydrogenase and 10 of immobilised NAD ⁺ reductase was suspended in 300/rL [ ² H5]-Tris. ² HCl (50 mM in ² ¾0, p ² H 8.0) containing 5 mM NADP ⁺ which had been pre-saturated with ¾ gas. The reaction solution was subsequently sealed in a pressure vessel under 2 bar of ¾ and rocked at 30 rpm for 16 hours at 20 ^° C.

Product analysis as described in Example 1 A showed a conversion of around 20 % to NADPH, with high selectivity (> 95 %) for the [45- ² H] -NADPH isotopomer (see Figures 13 A, 13B and 13C). The ¾ NMR spectra shown in Figure 13B and 13C were generated with the following parameters: 400 MHz, 64 scans, LB = 1.0 Hz, ² ¾0 (p ² H 8.0), 298 K. Two individual runs were pooled together to make a sample of the required volume and concentration.

Example 5

This Example provides a systematic comparison of various embodiments of the methods of the invention for production of [4- ² H]-NADH. Catalysts were screened for activity in converting NAD ⁺ to [ ² H]-NADH under various reaction conditions.

Experiments were carried out to screen the selectivity of H2-driven NAD ⁺ reduction by the routes illustrated in Figure 14. Experiments compared reduction of NAD ⁺ by (i) Pt/C (platinum supported on carbon); (ii) Pt+NAD-R/C (platinum and NAD ⁺ reductase (SEQ ID NO: 1,2,31,69) supported on carbon); (iii)

H2ase+NAD-R/C (E. coli hydrogenase 2 (SEQ ID NOs: 39-40) and NAD ⁺ reductase (SEQ ID NO:

1,2,31,69) supported on carbon) and (iv) soluble hydrogenase (SEQ ID NOs: 1,2,30,31) alone. The chemical, isotopic and stereo-selectivity under a number of ^x ¾ and ^x ¾0 conditions is reported in Table 1 below.

The heterogeneous catalysts were prepared as dispersions in aqueous buffer solution by sonication of either Pt/C (nominally 20 wt.%, Alfa Aesar) or carbon black (Black Pearls 2000, Cabot) at 20 mg mL ¹ . Enzyme- modified particles were prepared by pre-mixing the required enzyme solutions before adding dispersed carbon particle solution as described in Example 1 A. The particle-enzyme solutions were left at 4 °C for enzyme immobilisation. The heterogeneous systems were compared to a native enzyme, R. eutropha soluble hydrogenase (SEQ ID NOs: 1,2,30,31), which was added to reactions in solution.

The catalysts were injected into HL-saturated solution containing NAD ⁺ (4-5 mM) and left under 2 bar *¾ for 16 hours. The reactions were analysed using a combination of UV-vis spectroscopy, HPLC and NMR as described in Example 1A. Experiments were carried out on a small scale (500 pL) with low catalyst loading (100 m% carbon mL ¹ ). The mass of NAD ⁺ reductase exposed to the carbon particles was kept constant and unabsorbed enzyme was removed by centrifugation before use.

Initial experiments were performed in protiated solvent (¾0) and diprotium gas (¾) to evaluate the selectivity of the catalysts towards the formation of 4-NADH. For each system the chemo-selectivity refers to the concentration of 4-NADH generated relative to the loss of NAD ⁺ , as determined from HPLC traces (Table 1, Entries 1-4). Whilst the conversion of NAD ⁺ was of a similar magnitude for all catalysts (usually 60 - 90 %), the selectivity towards the formation of the desired 4-NADH was highly variable for the Pt/C system. For this latter case, yellowing of the reaction solution and appearance of extra peaks in subsequent HPLC analysis were evidence of the formation of biologically inactive side products (likely including NAD2 dimers, 2-/6-NADH, and over-reduced compounds) (Figure 15A). Such behaviour is in contrast to those catalysts bearing an NAD ⁺ reductase moiety, (Pt+NAD-R/C, H2ase+NAD-R/C and SH), which showed clean formation of only 4-NADH (Figure 15A). Without being bound by theory, the inventors believe that the high selectivity of the NAD ⁺ reductase is due to concerted H ⁺ + 2e (= H ) transfer from the flavin active site to the oxidised cofactor, preventing formation of radicals. The flavin and the NAD ⁺ are positioned such that hydride transfer only occurs to the 4 position on the nicotinamide ring thus only forming 4-NADH.

The Pt+NAD-R/C system also shows high selectivity for 4-NADH. This is particularly noteworthy, suggesting that there is rapid electron transfer from ¾ oxidation at Pt through the carbon particle to the NAD ⁺ reductase for selective NAD ⁺ reduction and that no unselective NAD ⁺ reduction at Pt occurs.

Analogous experiments were performed for each catalyst system with the same diprotium gas (¾) as the reductant, but with deuterated solvent, ² ¾0 (Table 1, Entries 5-8). The same selectivity as observed for NAD ⁺ reduction in ¾0 was recorded. The extent of ² H incorporation to generate [4- ² H]-NADH was analysed using NMR (Figure 15B). The % isotopic selectivity refers to [4- ² H]-NADH as a percentage of 4- NADH. The non-enzymatic Pt/C sytem shows a mixture of ¾ and ² H incorporation where Ή originates from ¾ gas (35 %) or the ² ¾0 solution (65 %), respectively. In contrast, in systems operating according to the methods of the invention (Pt+NAD-R/C, H2ase+NAD-R/C and soluble hydrogenase alone) the Ή is exclusively taken from solution. This provides evidence that the flavin active site in the first polypeptide combines electrons from the FeS cluster chain with ^X H ⁺ from solution and this hydride (Ή ) is selectively transferred to the oxidised cofactor, generating only [4- ² H]-NADH.

The high level of ² H incorporation observed for the Pt+NAD-R/C system further supports the observation that electrons from ¾ oxidation at Pt are rapidly transferred to the NAD ⁺ reductase for NAD ⁺ reduction as both the chemo and isotopic selectivity of the NAD ⁺ reductase are conserved.

Table 1: Catalyst screening for conversion of NAD ⁺ to [4- ² H]-NADH

Entr Catalyst Reductant Solvent®

1 Pt / C

2 AD ⁺ reductase / C

¾ ¾o

3 e + NAD ⁺ reductase / C

4(b) ble hydrogenase

5 Pt / C

6 AD ⁺ reductase / C

¾ ² H ₂ O

7 e + NAD ⁺ reductase / C

₈ (b) ble hydrogenase

/

E

Reactions conducted on 500 /iL scale with 4 mM NAD ⁺ under 2 bar gas pressure for 16 hours and rocking at 15 rpm (unless otherwise specified); (b) 5 mM NAD ⁺ ; (c) ¾0 = Tris-HCl (100 mM, pH 8.0), ² H ₂ 0 = ds- [ ² H ₅ ]-Tris. ² HCl (100 mM, pD 8.0); (d) Conversion refers to loss of NAD ⁺ _, as determined by HPLC ; (e) chemo-selectivity reported as the percentage of 4-NADH compared to the loss of NAD ⁺ , as determined by HPLC; (f) isotopic-selectivity reported as the percent of labelled 4-NADH compared to total 4-NADH, as determined by NMR; (g) stereo-selectivity for [45- ² H]-NADH compared to labelled 4-NADH, as determined by NMR; (h) overall yield of [4S- ² H]-NADH. Representative HPLC and NMR traces are shown in Figure 15A,B.

As expected, the results in Table 1 confirm that bare Pt shows very poor selectivity towards 4-NADH under any conditions. The results in Table 1 show that much higher yields of [45- ² H]-NADH are achieved using the Pt+NAD-R/C, H2ase+NAD-R/C and soluble hydrogenase systems according to the methods of the invention than are achieved using the purely chemical Pt/C system. The reduced labelled cofactor, [4- ² H]-NADH, can be formed as either the R- or S- stereoisomer, and the stereochemistry of the reduced cofactor can be assigned using NMR as described above. The results summarised in Table 1 demonstrate that the purely chemical Pt/C system gives a roughly racemic product.

By contrast, all the systems using the NAD ⁺ reductase for NAD ⁺ reduction in accordance with the methods of the invention selectively generate [45- ² H]-NADH.

Without being bound by theory, the inventors believe that the stereoselectivity of the biological systems using NAD ⁺ reductase for NAD ⁺ reduction in accordance with the methods of the invention is a consequence of the structure of the active site of the enzyme. Inspection of the crystal structure of the structurally similar protein, Complex 1 from Thermus thermophilus ( Tt ) and comparison with a homology model of the R.

eutropha HoxFU protein (SEQ ID NOs: 1,2) (Figure 16) shows the interaction of the NAD ⁺ reductase flavin active site and the reduced cofactor and provides evidence that a hydride from the FMN cofactor contained in the protein would be transferred to the .« ^' -face of the nicotinamide ring to preferentially generate [45- ² H]- NADH.

Example 6

This Example confirms that the isotopic composition of the reaction medium (rather than the reductant) determines the isotopic composition of the reaction product.

The mechanisms of [4- ^x H]-NADH generation by the heterogeneous systems described in Example 5 were further probed by comparing Ή incorporation under either ¾ or ² H2 in a series of ¾0: ² H2q mixtures (100:0, 75:25, 50:50, 25:75, and 0:100 v/v %).

Experiments compared reduction of NAD ⁺ by (i) Pt/C (platinum supported on carbon); (ii) Pt+NAD-R/C (platinum and NAD ⁺ reductase (SEQ ID NOs: 1,2,31,69) supported on carbon) and (iii) H2ase+NAD-R/C ( E . coli hydrogenase 1 (SEQ ID NOs: 37-38) and NAD ⁺ reductase (SEQ ID NOs: 1,2,31,69) supported on carbon). The isotopic selectivity under a number of ^c ¾ and Ή2O conditions is reported in Figure 17.

The required solution were prepared by mixing solutions of Tris-HCl (100 mM, pH 8.0) in ¾0 with [ ² ¾]- Tris. ² HCl (100 mM, pD 8.0) in ² ¾0 in the appropriate volumes. The catalysts were injected into ^x H2-saturated solution containing NAD ⁺ (4 mM) and left under 2 bar Ή2 for 16 hours. Experiments were carried out on a small scale (500 pL) with low catalyst loading (100 m% carbon mL ¹ ). The reactions were analysed using a combination HPLC and NMR as described in Example 1 A. The yield of reduced cofactor (of any isotopic composition) was between 50 - 90 mol% in all cases. The % ² H incorporation was determined by comparison of the relative intensities of the peaks corresponding to [45- ² H]-NADH, [4R- ² H]- NADH, and [4- ¹ H ₂ ]-NADH in the H NMR spectrum. The results in Figure 17 show that in the methods of the invention, ² H incorporation for systems including a NAD ⁺ reductase as the first polypeptide exclusively reflects the ratio of ² H: ¹ H available in the solvent (black diamonds and light grey squares). In contrast, the purely chemical system (Pt/C) (grey triangles) shows a strong bias towards incorporation of ¾ under all conditions.

The results in Figure 17 show that the Pt/C system is complex and non-selective in its behaviour, taking the Ή moiety from both the reductant gas and the reaction solution. Consequently, for the Pt/C system, 100 %

² H incorporation into the NADH can only be achieved when both 100 % ² ¾0 solvent and 100 % ² ¾ gas are both employed. In contrast, the biological systems operating in accordance with the methods of the invention take the Ή label entirely from the reaction medium. Surprisingly, the results also show that production of [4- ² H]-NADH is as effective with ² ¾ as the reductant as it is with ¾.

This Example thus shows that in the methods of the invention, the isotopic composition of the reaction medium (rather than the reductant) determines in all cases the isotopic composition of the reaction product.

A desired ratio of labelled: unlabelled cofactor can therefore be achieved by controlling the isotopic composition of the reaction medium.

Example 7

This Example demonstrates that the methods of the invention can be used to supply labelled cofactor to a NAD(P)H-dependent oxidoreductase in order to generate a chemo- and stereo-selectively labelled product. Four examples are used to verify that the methods of the invention are capable of generating and recycling deuterium-labelled cofactors to drive two alcohol dehydrogenases (Johnson Matthey ^-selective ADH101 and S-selective ADH 105), an ene reductase (Johnson Matthey ENE 107) and an amino acid dehydrogenase (Sigma L-alanine dehydrogenase) in the conversion of unlabelled substrate to labelled product.

Firstly, an ^-selective ADH and an S-selective ADH (ADH 101 and ADH 105 respectively) were used to deliver a deuteride to opposing faces of acetophenone, thereby separately generating both enantiomers of [¾]- phenyl ethanol.

Reactions were carried out using around 100 <g(C) catalyst with 10 - 20 m% ofE. coli hydrogenase 1 (SEQ ID NOs: 37-38) and I64A (SEQ ID NOs: 1,2,31,69) prepared according to the methodologies in Example 1). The catalyst was added to 500 /<L of [ ² H5]-Tris. ² HCl (100 mM, p ² H 8.0) containing 0.1 mM NAD ⁺ , 10 mM acetophenone, and 5 vol.% [ ² H5]-DMSO pre-saturated with ¾ gas. 0.5 mg of the required alcohol dehydrogenase was then added and the reaction solution was sealed in a shaker plate under a steady stream of ¾ and shaken at 750 rpm for 20 hours at 20°C. The reaction was analysed qualitatively by ¾ NMR and extracted into heptane for chiral HPLC (Figures 18Ai and 18Bi). The HPLC shows that the conversion has taken place and that the correct enantiomers have been produced ( R - for ADH101 and S- for ADH105). The absence of a multiplet peak at d = 4.91 ppm in the ¾ NMR spectrum, and collapse of coupling in the peak at d = 1.47 ppm (relative to 'H-standard), are diagnostic of the correct isotopologue having been produced (Figures 18Aii and 18Bii). Both methods of analysis indicate that the conversions are greater than 50 % and selectivity for the desired deuterated enantiomer are > 95 %. Such results indicate a cofactor turnover of > 50.

A second reaction was tested employing an ene-reductase, to further demonstrate the chemoselectivity of the invention by the reduction of a C=C in the presence of C=0. In this reaction dimethyl itaconate was converted to dimethyl [2- ² H]- 2-([ ² Hi]methyl) succinate. The reactions conditions were 200 <g(C) catalyst with 5 - 10 /ig of E. coli hydrogenase 1 (SEQ ID NOs: 37-38) and I64A (SEQ ID NOs: 1,2,31,69) co immobilised on it (prepared as above). 500 /<L of [ ² H5]-Tris. ² HCl (100 mM, p ² H 8.0) containing 0.5 mM NAD ⁺ , 5 mM dimethyl itaconate, and 2 vol.% [ ² ¾]-DMSO presaturated with ¾ gas charged with the catalyst. 0.5 mg of ene reductase was added and the reaction solution was sealed in a shaker plate under a steady stream of ¾ and shaken at 500 rpm for 16 hours at 20°C.

The reaction was analysed qualitatively by ¾ NMR and extracted into EtOAC for GC (Figure 18C). The GC shows that the conversion has taken place. The absence of a multiplet peak at d = 2.95 ppm, and collapse of coupling in peaks at d = 2.62 ppm and d = 1.19 ppm in the ¾ NMR spectrum (relative to 'H-standard), are diagnostic of the correct isotopologue having been produced. Both methods of analysis indicate that the conversions are around 20 % and selectivity for the desired deuterated enantiomer are > 90 %. Such results indicate a cofactor turnover of around 4.

Finally, a reaction was conducted to demonstrate the ability of the catalyst in a reductive amination reaction, involving the conversion of an alpha-keto acid (pyruvate) to a deuterated amino acid ([2S'- ² H]-alanine). In these reactions 400 <g(C) catalyst with 20 - 40 mg of hydrogenase 1 (SEQ ID NOs: 37-38) and I64A (SEQ ID NOs: 1,2,31,69) co-immobilised on it (prepared as above). 500 /<L of [ ² Hn]-Tris. ² HCl (100 mM, p ² H 8.0) containing 0.5 mM NAD ⁺ , 5 mM sodium pyruvate, and 25 mM NFLCl was presaturated with ¾ gas and charged with the catalyst. 0.5 mg of L-alanine dehydrogenase was added and the reaction solution was sealed in a shaker plate under a steady stream of ¾ and shaken at 500 rpm for 16 hours at 20°C.

The reaction was analysed qualitatively by ¾ NMR. The absence of a multiplet peak at d = 3.83 ppm, and collapse of coupling in the peak at d = 1.45 ppm in the ¾ NMR spectrum (relative to 'H-standard), are diagnostic of the correct isotopologue having been produced (see Figure 18D). The complete disappearance of the peak corresponding to the pyruvate starting material (which remained in the control experiment) indicates that the conversion to alanine is high, with the maximum cofactor turnover of 10 having been achieved. The selectivity for [2S'- ² H]-alanine appears also to be high (around 85 %). A summary of the reactions demonstrated is shown in Figure 18E.

Example 8

This Example demonstrates that the methods of the invention can be used to synthesize a range of labelled cofactors.

The results above demonstrate that the methods of the invention can selectively generate the S isomer of the deuterium labelled cofactor, (i.e. [4 _I 5- ² H]-NADH, and that this cofactor can be used by an ^-selective alcohol dehydrogenase (ADH) for reductive deuterium addition to a ketone. However, for a number of applications for examples in mechanistic studies it is desirable to have access to other deuterium labelled cofactors.

Figure 19 details routes to [4- ² H]-NA(P)D ⁺ , [4- ² H]-NAD(P)H, [4/T ² H]-NAD(P)H, and [4S- ² H]-NAD(P)H using the methods of the invention. [4 _I 5- ² H]-NAD(P)H can be obtained from NAD ⁺ using the methods of the invention described above. If [45- ² H]-NAD(P)H is provided to a S-selective oxidoreductase, the ² H label is not incorporated into the reduced product (Figure 19, Step B), and the resulting cofactor is the labelled oxidised cofactor, [4- ² H]-NA(P)D ⁺ . The labelled oxidised cofactor can be further reduced using the methods of the invention to obtain the doubly-reduced cofactor, ([4- ² H ₂ ]NAD(P)H (Figure 19, step D). Alternatively, analogous methods to those of the invention but conducted in unlabelled solvent (e.g. ¾0) can be used to reduce the labelled oxidised cofactor, [4- ² H]-NA(P)D ⁺ to generate [4/?- ² H]NAD(P)H (Figure 19, step C). If the oxidoreductase used is immobilised on a solid surface such as carbon particles it can be easily removed from solution e.g. by filtration leaving the organic product and any unreacted reactants behind. The desired cofactor can easily be isolated by evaporation of the aqueous solution. The absence of labelled reductant in solution significantly simplifies isolation of the cofactors after each step.

The above methods were demonstrated using the H2ase+NAD-R/C system for selective NAD ⁺ reduction. This system was chosen due to its selectivity and the ease of separation of the catalyst from the reaction mixtures. Any of the systems in accordance with the methods of invention can be used to generate the cofactors.

The general scheme shown in Figure 19 was used to prepare different isotopologues of NADH (in oxidised and reduced forms). In brief, after preparing [4 _I 5- ² H]-NADH according to the methods of the invention, the [4 _I 5- ² H]-NADH was re-oxidised by reaction with excess AcPh and an immobilised ADH105 (an S-selective enzyme), to leave [4- ² H]-NAD ⁺ . Following removal of unreacted ADH101 (an ^-selective enzyme) and the side-product PhEtOH, the [4- ² H]-NAD ⁺ was transferred to either ¾0 or ² ¾0 solutions. Further reduction using the H2ase+NAD-R/C system in the presence of ¾, yielded the cofactors [4- ² H ₂ ]-NADH (when a ² ¾0 solvent was used) and [4/?- ² H]-NADH (when a ¾0 solvent was used), respectively. The following conditions were used in the reactions (using Figure 19 for step labels):

Step A: Synthesis of [4A- ² H]-NADH from [4- ¹ H]-NAD ⁺

100 /ig(C) catalyst with 20 - 40 m% oΐE. coli hydrogenase 1 (SEQ ID NOs: 37-38) and I64A (SEQ ID NOs: 1,2,31,69) co-immobilised on it (prepared as previously) was added to 500 mE of [ ² ]¾]-Tris. ² HCl (100 mM, p ² H 8.0) containing 4 mM NAD ⁺ , which had been presaturated with ¾ gas. The reaction solution was sealed under 2 bar ¾ for 16 hours, whilst rocking at 30 rpm. Analysis by UV-spectrophotometry and ¾ NMR spectroscopy indicated complete conversion of the cofactor to the desired [45- ² H]-NAOH form.

Step B: Synthesis of [4- ² H]-NAD ⁺ from [4A- ² H]-NADH

Johnson Matthey alcohol dehydrogenase (ADH105) was immobilised on carbon particles by suspending a concentrated solution (20 mg/mL) in an equal volume of sonicated BP2000 particles (20 mg/mL) for 30 minutes at 4 °C. Following centrifugation (12 000 rpm, 5 minutes) the supernatant was removed, and the particles washed once in 100 mE ² H2q. The ADH particles were then added to a deoxygenated solution of [45- ² H]-NADH (1 mL, 4 mM) in [ ² H5]-Tris. ² HCl (100 mM, p ² H 8.0), followed by neat acetophenone (10 mM), and the whole solution was shaken under N2 for a period of 5 days. The ADH particles were removed by centrifugation (12 000 rpm, 5 minutes) and the sacrificial acetophenone / phenylethanol removed by extraction with C ² HCl3 (3 ^c 500 /rL). Analysis by UV-spectrophotometry and ¾ NMR spectroscopy indicated > 90 % conversion of the cofactor to the desired [4- ² H]-NAD ⁺ form, with the absence of a doublet at S = 8.8 ppm being evidence of the labelling at the 4-position.

Step C: Synthesis of [4- ² H ₂ ]-NADH from [4- ² H]-NAD ⁺

Particles of the same constitution as Step A were added at a loading of 200 /ig(C)/mL to a solution of [4-¾ ₂ ]- NADH (500 /iL, 3 mM) that had been pre-saturated with ¾ gas. The solution was then sealed under 2 bar ¾ and rocked at 30 rpm for 16 hours. Analysis by UV-spectrophotometry and ¾ NMR spectroscopy indicated > 90 % conversion of the cofactor to the desired [4-¾ ₂ ]-NAD ⁺ form, with the relative absence of signals at d = 2.6 - 2.8 ppm being evidence of the complete labelling.

Step D: Synthesis of |4/?- ² H]-NADH from [4- ² H]-NAD ⁺

A solution of [4- ² H]-NAD ⁺ (l mL, 3 mM) in [ ² H5]-Tris. ² HCl (100 mM, p ² H 8.0) was prepared according to Step B, except using free alcohol dehydrogenase (rather than immobilised). To the solution was added an equal volume of acetonitrile, and precipitated alcohol dehydrogenase removed by centrifugation (12 000 rpm, 5 minutes). The solution was gently evaporated to dryness on a rotary evaporator, and the solid re-dissolved in deionised ¾0. The evaporation and re-dissolution steps were repeated twice more. The solution was evaporated a final time, before being transferred to a glovebox and being re-dissolved in deoxygenated deionised ¾0 (1 mL). The cofactor solution was subsequently saturated with ¾ gas. 200 mgC catalyst with 30 - 40 /ig of E. coli hydrogenase 2 (SEQ ID NOs: 39,40) and NAD ⁺ reductase immobilised on the surface was added to solution, which was subsequently sealed under 2 bar ¾ and shaken at 30 rpm for 18 hours. The carbon catalyst was removed by centrifugation (12 000 rpm, 5 minutes) and the solution analysed by UV- spectrophotometry and ¾ NMR spectroscopy. The analysis indicated around 60 % conversion to the reduced cofactor, with a high selectivity (> 90 %) for the [4R- ² H]-NADH form, as evidence by the signal at S = 2.66 ppm.

Each of the cofactors produced was analysed using UV-vis spectroscopy and NMR as described in Example 1A. Data are shown in Figure 20.

Example 9

This Example provides further verification that the methods of the invention can be used to supply labelled cofactor to a NAD(P)H-dependent oxidoreductase in order to generate a chemo- and stereo-selectively labelled product.

In the results discussed below, the % ² H incorporation achieved at the target sites using this approach was between 93-99%. The demonstrated ability to work across diverse functional group space indicates the utilty of this approach to generate libraries of well-defined [¾]- labelled chiral building blocks, e.g. for fine chemical synthesis, for small molecules for analytical applications, or for later-stage deuteration of pharmaceutical precursors, particularly where biocatalysis is already implemented in the reaction sequence.

All experiments in this Example were conducted using the biocatalyst system of the invention with E. coli hydrogenase 1 (SEQ ID Nos: 37-38) and NAD ⁺ reductase I64A (SEQ ID Nos: 1,2,31,69) prepared as described above. Commercial enzymes were received in lyophilized form and used without further purification. Catalyst system was prepared by sonication of a 20 mg/mL suspension of BP2000 carbon black in Tris-HCl buffer for 5 ^c 15 minutes (with agitation of the solution in between). Equal volumes of hydrogenase (4 mg/mL) and NAD ⁺ reductase (1.4 mg/mL) were then pre-mix ed together, and added immediately to an aliquot of sonicated carbon. After standing at 4 °C for 60 minutes, the solid catalyst was then removed from the preparatory solution by centrifugation (10, 000 ^x g, 5 mins) before being re suspended in deuterated or non-deuterated buffer as required. Enzyme loadings: hydrogenase loading of 39 pmoles per 100 mg of carbon, NAD ⁺ reductase loading of 65 pmoles per 100 mg of carbon.

Deuterated buffer ( ² H ₅ )-Tris- ² HC1 was prepared by dissolving the required amount of Trizma® base in ¾ q and then evaporating to dryness. After repeating twice more, the pD (p ² H) of the Tris solution was adjusted to 8.0 by the addition of small aliquots of ² HC1 (3.0 M) prior to deoxygenation by sparging with dry N . Solutions of fully deuterated ( ² Hn)-Tris- ² HCl were also used for analytical purposes, and were prepared in a similar manner. ¾ NMR spectroscopy indicated that the final %¾ q of deuterated buffer solutions was not below 99 mol.% (unless specifically diluted with ¾()). Other conditions and analysis conducted as described above unless otherwise stated.

GC-FID was carried out on a ThermoScientific Trace 1310. GC-MS was carried out on an Agilent 7890B GC coupled to an Agilent 7200 Accurate Mass Q-ToF MS operating under El mode. For both machines, injections were carried out by means of a robotic autosampler. The relevant columns and chromatography conditions are stated as required.

All HPLC was conducted on a Shimadzu UFLC LC-20AD Prominence liquid chromatograph equipped with a dual wavelength UV-spectrophotometric detector and a robotic autosampler. MilliQ water and HPLC grade solvents were used throughout. The relevant columns and chromatography conditions are stated as required.

Example 9.1

In this reaction pyruvate was converted to [2L- ² H]-lactate. The reactions were conducted in 0.5 mL of ( ² Hn)-Tris- ² HCl (100 mM, p ² H 8.0) containing 5 mM sodium pyruvate, 0.5 mM NAD ⁺ , and 500 pg of L- lactate dehydrogenase (Merck). The mixture was presaturated with ¾ gas prior to addition of the heterogeneous biocatalytic system at a loading of 400 pg. The reactions were shaken at 500 rpm under a steady flow of ¾ for 16 hours. The reaction was analysed by GC, MS and NMR.

GC-FID: analytes were first derivatised and then subjected to analysis by GC-FID. 100 pL of reaction mixture was combined with 23 pL of EtOH and 13 pL of pyridine by means of a vortex mixer. Subsequently, 15 pL of ethyl chloro formate was added, and the reaction allowed to proceed until no further CO2 was evolved. The derivatised pyruvate/lactate was extracted with 100 pL of C ² HCl3, and transferred to a glass vial for analysis by GC. Conditions as below:

Column: DB-1701 (Agilent), 30 m length, 0.25 mm diameter, 0.25 pm film thickness; Carrier: He (CP grade), 1.1 mL minute (constant flow); Inlet temperature: 250 °C; Injection conditions: Splitless with split flow 50 mL/min, splitless time 0.7 mins, purge 5 mL/min; Injection volume: 0.5 pL; Detection: FID; Detector temperature: 200 °C; Detection gases: ¾ (35 mL/min), air (350 mL/min), makeup N2 (40 mL/min); Oven heating profile:

0-2 mins, Hold at 45 ^° C

2-15 mins, Ramp to 250 °C at 16 °C/min

15-20 mins, Hold at 250 °C for 5 mins

Chiral GC-FID: The ee of the lactate product was determined by first derivatising with a chiral alcohol ((2R,3R)-(-)-2,3-butanediol) and then analysing the reaction solution by GC-FID. 100 pL of reaction mixture was combined with 35 pL of (2R,3R)-(-)-2,3-butanediol and 13 pL of pyridine by means of a vortex mixer. Subsequently, 15 pL of ethyl chloro formate was added, and the reaction allowed to proceed until no further CO2 was evolved. Commercial standards of L- and D-lactate were similarly derivatised for comparison. The derivatised analytes were then extracted with 100 /<L of C ² HCl3, and transferred to a glass vial for analysis by GC. The formation of diastereomeric products allowed for the analysis to be conducted on an achiral GC column. Conditions as below:

Column: DB-1701 (Agilent), 30 m length, 0.25 mm diameter, 0.25 pm film thickness; Carrier: He (CP grade), 170 kPa (constant pressure); Inlet temperature: 230 °C; Injection conditions: Splitless with split flow 50 mL/min, splitless time 0.7 mins, purge 5 mL/min; Injection volume: 0.5 pL; Detection: FID; Detector temperature: 250 °C; Detection gases: ¾ (35 mL/min), air (350 mL/min), makeup N2 (40 mL/min); Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 100°C

5 30 Ramp to 150 °C at 2 °C/min

30 35 Hold at 150°C for 5 minutes

35 41.5 Ramp to 280 °C at 2 °C/min

41.5 46.5 Hold at 280 ^° C for 5 minutes

GC-MS: Following analysis by GC-FID the EtOH/ethyl chloro formate derivatised reaction solutions were further analysed by GC-MS according to the method shown below. A commercial sample of sodium lactate of natural isotopic abundance was derivatised and analysed in an identical manner for comparison.

Conditions as below:

Column: DB-1701 (agilent), 30 m length, 0.25 mm diameter, 0.25 /an (film thickness); Carrier: He (CP grade), 100 kPa (constant pressure); Inlet temperature: 250 °C; Injection conditions: Split (10:1) with split flow 12 mL/min, splitless time 0.7 mins, purge 5 mL/min; Detection: Mass Spec, El (70 eV), source temperature 230 °C. Scan range 50 - 650 amu with a scan rate of 5 Hz. Transfer line 300 °C.; Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 50 ^° C

5 16.3 Ramp to 275 °C at 20 °C/min

16.3 18.8 Hold at 275 °C for 2.5 mins

H NMR spectroscopy: After removal of the catalyst, the unmodified reaction solutions were analysed by ¾ NMR spectroscopy at 500 MHz and 298 K.

Results are shown in Figure 21.

The very high conversion of pyruvate to lactate was confirmed by GC-FID analysis of the derivatised reaction solution (see Figure 21(a)(ii)). Here, the peak corresponding to the pyruvate starting material (detected as ethyl pyruvate, RT = 5.85 minutes) disappeared almost entirely in the bio-hydrogenation reaction compared to a control in which no catalyst was included. The appearance of a peak at RT = 12.55 minutes, corresponding to the derivatised form of lactate, provided confirmation that the reaction had proceeded to 95 % completion. Similarly, derivatisaition of L- and D- lactate with a second chiral alcohol affords diastereomeric products with differing retention times {L = 25.5 mins, R = 25.3 mins, see Figure 21 (b)(ii)). Hence, by comparison, it could be confirmed that the lactate produced in the biohydrogenation was entirely of the T-form, within the limits of detection (> 99 %). The site and extent of ² H labelling on the L- lactate product was determined through a combination of GC-MS and ¾ NMR spectroscopy, Figure 21(c) and (d), respectively. In the ¾ NMR spectrum, the signal corresponding to the -C¾ protons could be used to detect ² H labelling on the a-carbon of T-lactate, forming a doublet (S = 1.34 ppm, J= 9.2 Hz) when a ¾ nucleus was at the a-position, and a broad singlet (S = 1.34 ppm) when a ² H was present. Similarly, a quartet (S = 4.13 ppm, J= 8.7 Hz) corresponding to the a-'H signal was present in non-deuterated samples, but absent in those with a ² H-label. Deuterium exchange on the -C¾ group to yield -CH2 ² H was also evidenced by a smaller, broad shoulder at d = 1.32 (although it is not possible to determine the extent of complete deuterium exchange of the -C¾ group via this method). Analysis of the ethoxycarbonyl ethylester derivatised lactate by mass spectroscopy gave a series of diagnostic peaks, notably the molecular ions at m/z = 190.1 [CsHisOs^] and m/z = 191.1 H-CsHuOs "], which could be used to determine the extent of ² H incorporation at the a-position as > 97 %. The peak at m/z = 192.1 could also be used to estimate the extent of formation of [ ² H2-CsHi305 ^+’ ] (Figure 21 (e)).

Example 9.2

In this reaction phenylpyruvate was converted to [2,3- ² H ₃ ]-L-phenylalanine. Phenylpyruvic acid (5 mM) in 0.5 mL of ( ² Hn)-Tris- ² HCl (100 mM, p ² H 8.0) was first allowed to stand for 24 hours in order to exchange labile protons for deuterons, before the addition of 25 mM NFfiCl, 0.5 mM NAD ⁺ , and 500 m of L- phenylalanine dehydrogenase. The mixture was presaturated with ¾ gas prior to addition of the Bio-catalyst systems at a loading of 400 m%. The reaction was then shaken at 500 rpm under a steady flow of ¾ for 16 hours.

GC-FID: In order to determine the conversion of phenylpyruvate to alanine, the analytes were first derivatised and then subjected to analysis by GC-FID. 100 mE of reaction mixture was combined with 23 mE of EtOH and 13 mE of pyridine by means of a vortex mixer. Subsequently, 15 mE of ethyl chloro formate was added, and the reaction allowed to proceed until no further CO2 was evolved. The derivatised

pyruvate/alanine was extracted with 100 mE of C ² HCl3, and transferred to a glass vial for analysis by GC. Conditions as below:

Column: DB-1701 (Agilent), 30 m length, 0.25 mm diameter, 0.25 pm film thickness; Carrier: He (CP grade), 170 kPa (constant pressure); Inlet temperature: 230 °C; Injection conditions: Splitless with split flow 50 mL/min, splitless time 0.7 mins, purge 5 mL/min; Injection volume: 0.5 pL; Detection: FID; Detector temperature: 250 °C; Detection gases: ¾ (35 mL/min), air (350 mL/min), makeup N (40 mL/min); Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 100°C

5 30 Ramp to 150 °C at 2 °C/min

30 35 Hold at 150°C for 5 minutes

35 41.5 Ramp to 280 °C at 2 °C/min

41.5 46.5 Hold at 280 ^° C for 5 minutes

GC-MS: The N-ethoxycarbonyl ethylester-derivatised samples from the GC-FID analysis described (see above) were subsequently analysed by GC-MS according to the method below. A commercial sample of L- phenylalanine of natural isotopic abundance was derivatised and analysed in an identical manner for comparison. Conditions as below: Column: DB-1701 (agilent), 30 m length, 0.25 mm diameter, 0.25 /on (film thickness); Carrier: He (CP grade), 100 kPa (constant pressure); Inlet temperature: 250 ^° C; Injection conditions: Split (10:1) with split flow 12 mL/min, splitless time 0.7 mins, purge 5 mL/min; Detection: Mass Spec, El (70 eV), source temperature 230 ^° C. Scan range 50 - 650 amu with a scan rate of 5 Hz. Transfer line 300 °C.; Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 50 ^° C

5 16.3 Ramp to 275 °C at 20 °C/min

16.3 18.8 Hold at 275 °C for 2.5 mins

Chiral GC-FID: Derivatisation of the samples for analysis by chiral GC-FID to establish the enantiomeric excess of the reaction, was carried out as described above, except with «PrOH (30 /<L) substituted for EtOH. Chiral GC-FID was then carried out according to the following method. Conditions as below:

Column: CP-Chirasil-Dex CB (Agilent), 25 m length, 0.25 mm diameter, 0.25 /an (film thickness), fitted with a guard of 10 m undeactivated fused silica of the same diameter; Carrier: He (CP grade), 2 mL/min (constant flow); Inlet temperature: 200 °C; Injection conditions: Splitless with split flow 80 mL/min, splitless time 0.8 mins, purge 5 mL/min.; Injection volume = 0.3 «L; Detection: FID; Detector temperature: 200 °C; Detection gases: ¾ (35 mL/min), air (350 mL/min), makeup N (40 mL/min); Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 70 ^° C

5— 115 Ramp to 180 °C at TC/min

115 130 Hold at 180 °C for 15 minutes

H NMR spectroscopy: After removal of the catalyst, the unmodified reaction solutions were analysed by ¾ NMR spectroscopy at 500 MHz and 298 K. Results are shown in Figure 22.

The very high conversion of phenylpyruvate to phenylalanine was confirmed by GC-FID analysis of the derivatised reaction solution (see Figure 22(a)(ii)). Here, the peak corresponding to the derivatised phenylpyruvate starting material (RT = 15.05 minutes) disappeared almost entirely in the bio-hydrogenation reaction compared to a control in which no catalyst was included. The appearance of a peak (RT = 14.94 minutes) corresponding to the N-ethoxycarbonyl ethylester derivatised form of phenylalanine, provided confirmation that the reaction had proceeded to > 99 % completion. Similarly, derivatisation of commercial standards of L- and D-phenylalanine and analysis on a chiral GC-column gave rise to two peaks ( L = 91.78 minutes, D = 92.00 minutes, see Figure 22(b)(ii)). Hence, it could be confirmed that the alanine produced in the biohydrogenation was entirely of the T-form, within the limits of detection. The site and extent of ² H labelling on the T-phenylalanine product was determined through a combination of GC-MS and ¾ NMR spectroscopy (see Figure 22 (c) and (d) respectively). In this case, the phenylpyruvate starting material was left in the reaction solution to allow exchange of the labile protons for deuterons in the solvent. Following reduction by the biocatalyst system and T-phenylalanine dehydrogenase, the resulting product was labelled on both a- and //-positions. Accordingly, the signals at d = 4.01 ppm (dd, 1H, aH, J= 4.1 Hz, J= 6.2 Hz), d = 3.31 ppm (dd, 1H, ^H, J= 4.1 Hz, J= 11.7 Hz), and d = 3.14 ppm (dd, lH, /H, ./= 6.4 Hz, J= 11.7 Hz) which were all observed in the commercial standard of T-phenylalanine, were found to be absent in the reaction product. Similarly, GC-MS analysis of the ethoxycarbonyl ethylester-derivative of phenylalanine demonstrated the expected +3 mass shift of the molecular from m/z 220.1 to 223.1 (see Figure 22 (c)).

Example 9.3

In this reaction cinnamaldehyde was selectively deuterated using alcohol dehydrogenase (reaction A), ene reductase (reaction B), or both ene reductase and subsequently alcohol dehydrogenase (reaction C).

Cinnamaldehyde was used as a substrate (bearing an alpha, beta-unsaturated aldehyde moiety) to investigate the chemoselectivity of the H2-driven labelling strategy. Conventional hydrogenation of this substrate typically results in a mixture of products (hydrocinnamaldehyde, cinnamyl alcohol and 3-phenyl- 1 -propanol) (56), however, by using either an ene reductase or an alcohol dehydrogenase alone, or the two enzymes in a step-wise one-pot reaction, the results below demonstrate that high chemical control over the deuterium- labelled product could be achieved.

Reactions were conducted in 0.5 mL of ( ² Hn)-Tris- ² HCl (100 mM, p ² H 8.0) containing 5 mM

cinnamaldehyde, 2 vol.% DMSO, 0.5 mM NAD ⁺ , and 500 m of (A) alcohol dehydrogenase (JM, ADH 105), and (B-C) ene reductase (JM, ENE101). The mixture was presaturated with ¾ gas prior to addition of the heterogeneous biocatalytic system at a loading of 400 m%. The reactions were shaken at 500 rpm under a steady flow of ¾ for 16 hours. In the case of reaction C, the initial step was allowed to proceed for 24 hours before addition of a further 200 m% of the heterogeneous biocatalytic system and 500 m% of alcohol dehydrogenase (JM, ADH 105).

GC-FID: Following the reactions, an aliquot of the solution was extracted with a 2 x volume of C ² HCl3, and then centrifuged at 18 800 x g for 5 minutes before being transferred to glass vials for analysis by GC-FID according to the method below. Column: DB-1701 (Agilent), 30 m length, 0.25 mm diameter, 0.25 /an film thickness; Carrier: He (CP grade), 0.5 mL minute (constant flow); Inlet temperature: 230 ^° C; Injection conditions: Splitless with split flow 60 mL/min, splitless time 0.8 mins, purge 5 mL/min; Injection volume: 0.5 uL Detection: FID; Detector temperature: 150 °C; Detection gases: ¾ (35 mL/min), air (350 mL/min), makeup N2 (40 mL/min); Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 50 ^° C

5 25 Ramp to 250 °C at 10 °C/min

25 35 Hold at 250 °C for 10 mins

GC-MS: Following extraction and analysis by GC-FID (above) the reaction solutions were analysed by GC- MS according to the method below. Column: DB-1701 (agilent), 30 m length, 0.25 mm diameter, 0.25 /on (film thickness); Carrier: He (CP grade), 100 kPa (constant pressure); Inlet temperature: 250 ^° C; Injection conditions: Split (25:1) with split flow 30 mL/min, splitless time 0.7 mins, purge 5 mL/min; Detection:

Mass Spec, El (70 eV), source temperature 230 ^° C. Scan range 50 - 650 amu with a scan rate of 5 Hz; Transfer line 300 °C.; Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 50 ^° C

5 16.3 Ramp to 275 °C at 20 °C/min

16.3 18.8 Hold at 275 °C for 2.5 mins

H NMR spectroscopy: After removal of the catalyst, the unmodified reaction solutions were analysed by ¾ NMR spectroscopy at 500 MHz and 298 K. In the case of reactions A and C, it was necessary to acquire additional spectra under non-aqueous conditions by extracting the product into an equal volume of C ² HCL and re-analysing it.

The results for reactions A, B, and C are shown in Figures 23, 24 and 25, respectively.

A: [l- ² H]-cinnamyl alcohol

Analysis by GC-FID, Figure 23(a), shows a broad peak for the cinnamyl alcohol product (RT = 19.9 mins) and one for unreacted cinnamaldehyde (RT = 19.4 mins), with no additional products being detected (including hydrocinnamalehyde and 3 -phenyl- 1 -propanol, which are common side products in the hydrogenation of cinnamaldehyde). Integration of the peak areas compared to a set of standard solutions indicated a conversion of 90 %, which could be confirmed by comparison of clearly resolved peaks in the ¾ NMR spectrum of the crude reaction mixture (see Figure 23 (b)). The site and extent of ² H labelling in the cinnamyl alcohol product was determined through ¾ NMR spectroscopy, Figure 23 (b). The intensity of the doublet at S = 4.30 ppm (J= 5.5 Hz) in the unlabelled cinnamyl alcohol standard (corresponding to the a- protons) halves in intensity in the spectrum of the biocatalytic reaction product. Overlapping peaks from the ribose ring of the cofactor make a precise integration of the peak from the a-proton difficult, though extracting the product into C ² HCl3 and re-acquiring the spectrum enabled the measurement to be conducted unambiguously. Hence, it was confirmed that the a-site had been labelled with a single ² H nucleus.

Accordingly, the peak corresponding to the neighbouring C2 proton is also found to change from a doublet of triplets in the unlabelled standard (S = 6.47 ppm, dt, J= 16.1 Hz, J= 5.8 Hz), to a doublet of doublets in the deuterated product (d = 6.47 ppm, dd, J= 16.1 Hz, J= 5.8 Hz). Unfortunately, mass spectroscopic analysis could not be used to unambiguously evaluate the extent of % ² H labelling, as such compounds are known to re-arrange upon ionization, causing large differences in the fragmentation pattern of different isotopomers. However, the spectra were still acquired, and are shown in Figure 24(c) for completeness. Here, the molecular ion peak in the commercial cinnamyl alcohol standard ([C ₉ H ₁₀ CU], m/z 134.1) is seen to increase by + 1.0 for the product of the biocatalytic hydrogenation, consistent with the addition of a ² H nucleus ([¾- C ₉ H ₉ CU], m/z 135.1).

B: [2, 3- ² H ₂ ] -hydrocinnamaldehyde

The near quantitative conversion of cinnamaldehyde to hydorcinnamaldehyde could was demonstrated by GC-FID analysis, see Figure 24 (a). Here, the cinnamaldehyde substrate (RT = 19.4 minutes) was absent from the reaction solution, which showed a peak only for hydrocinnamaldehyde (RT = 17.5 mins), without the formation of other possible side products (namely cinnamyl alcohol and/or 3 -phenyl- 1 -propanol). This result was further confirmed by ¾ NMR analysis of the crude reaction mixture (see Figure 24 (b)).

The site and extent of ² H labelling in the hydrocinnamaldehyde product could also be determined through ¾ NMR spectroscopy, Figure 24 (b), though the interpretation is complicated by the speciation of the molecule under aqueous conditions. As such, each of the aliphatic proton environments on the molecule (denoted a, b, and c in Figure 24 (b) give rise to three separate peaks in the corresponding ¾ spectrum, which must be summed together in order to determine the extent of ² H incorporation at each site. Accordingly, signals corresponding to sites a and b lose half of their intensity when the molecule is prepared by biocatalytic deuteration, whilst proton c (and the aromatic protons) remain unchanged. The extent of the collapse in coupling across all of the peaks is also commensurate with the addition of single deuterons at positions a and b. Unfortunately, mass spectroscopic analysis could not be used unambiguously to evaluate the extent of % ² H labelling as such compounds are known to re-arrange upon ionization, thereby causing large differences in the fragmentation pattern of different isotopomers. However, the spectra were still acquired, and are shown in Figure 24 (c) for completeness. Here, the molecular ion peak in the commercial standard of hydrocinnamaldehyde ([C ₉ H ₁₀ CU], m/z 134.1) is seen to increase by + 2.0 for the product of the biocatalytic hydrogenation, consistent with the addition of two ² H nuclei ([ ² H ₂ -0 ₉ ¾0 ⁺ ·], m/z 136.1).

C: [1, 2, 3 - H _. ] -3 -phenyl- 1 -propanol

The conversion of cinnamaldehyde to hydrocinnamaldehyde by the action of the heterogeneous biocatalytic system and an ene reductase was shown to proceed quantitiatively. The second half of Reaction C, in which the hydrocinnamaldehyde was reduced further to 3 -phenyl- 1 -propanol by the introduction of an alcohol dehydrogenase, was shown to proceed to a similarly high degree by GC-FID analysis (see Figure 25 (a)). Here, signals corresponding to the substrate (RT = 19.4 mins) and intermediate (RT = 17.5 mins) compounds were replaced in the chromatogram of the reaction mixture by the product peak (RT = 18.7 mins). Similarly, analysis of the ¾ NMR spectrum of the crude reaction mixture indicated that the reaction had proceeded to > 98 % conversion. Recovery of the product was not, however, quantitative, with around 30 % having been lost to evaporation over the course of the reaction. The site and extent of ² H labelling in the 3 -phenyl- 1 -propanol product was determined through ¾ NMR spectroscopy, Figure 25 (b). Analysis of the crude reaction mixture is complicated by the coincidence of the diagnostic peaks with those from other sources (such as the co solvent and buffer, see Figure 25 (b)(i)). As such, the product is better analysed by extracting into C ² HCl ₃ and re-acquiring the spectrum (see Figure 25 (b)(ii)). Here the intensity of signals corresponding to protons in position b (d = 2.72 ppm) and d (d = 3.68 ppm) are reduced by 50 % following the deuteration reaction (compared to a standard sample of natural isotopic abundance), consistent with the addition of a single deuteron at each of these sites. The signal for the proton at position c (S = 1.90 ppm) was found to decrease by 75 % however, indicating that 1.5 ² H units had been installed at this site. The additional ² H incorporation in this latter case most likely occurred through tautomeric solvent exchange following the reduction of the C=C double bond. Upon deuteration, the clear splitting patterns for peaks b (a pseudo- triplet), c (a pseudo- quintet), and d (a pseudo- quartet), are replaced by broad, poorly defined signals, consistent with the influence of much weaker proton-deuteron coupling. Mass spectroscopy was also used to study the isotopic substitution pattern along the 3 -phenyl- 1 -propanol product (see Figure 25 (c). Here the molecular ion peak was found to be diagnostic, with the m/z 136.1 representing the unfragmented molecule. Accordingly, peaks at m/z 137.1, 138.1, and 139.1, in the analysis of the reaction mixture could be attributed to the inclusion of two, three, and four ² H nuclei, respectively, consistent with the various levels of labelling on C2 described above.

Example 9.4

In this reaction carvones were selectively reduced to [l,2- ² H ₂ ]-dihydrocarvones using ene reductase Reactions were conducted in 0.5 mL of ( ² H ₅ )-Tris- ² HC1 (100 mM, p ² H 8.0) containing 5 mM (4R)-carvone (Reaction A) or (45)-carvone (Reaction B), 4 vol.% [ ² H5]-DMSO, 0.5 mM NAD ⁺ , and 500 m of ene reductase (JM, ENE 101). The mixture was presaturated with ¾ gas prior to addition of the heterogeneous bio-system at a loading of 400 m%. The reactions were shaken at 500 rpm under a steady flow of ¾ for 16 hours. Evaporation of the product dihydrocarvones proved to more problematic than in other cases so alternative reaction setups were trialled, including a pressure vessel (Biichi Tinyclave) sealed under 2 bar ¾ (50 mL headspace), and a reaction in a 1.5 mL glass GC-vial sealed under ¾ balloon pressure.

Whilst a commercial standard of mixed of (1R, 4 R)- and (15, 4R)-dihydrocarvone was commercially available, the 45-epimer was unavailable. Instead, this was synthesised by reduction of (45)-carvone by Zn metal. Here, Zn metal (625 mg, 9.6 mmol) and KOH (250 mg, 4.5 mmol) were combined in 3.5 mL of MeOH/H ₂ 0 (95/5 v/v) and the slurry bought to reflux under stirring. (45)-carvone (500 mg, 3.3 mmol) was dissolved in 1 mL of MeOH/H ₂ 0 (95/5 v/v) and added dropwise to the Zn-solution over 6 hours. Following the reaction, the solution was filtered through a syringe filter, extracted into pentane (3 >< 1 mL) and dried over Na2SC>4. The solvent was removed in vacuo to give (45)-dihydrocarvone (400 mg, 80 %) as a mixture of cis- 1,4 and tram-1,4 epimers in the ratio 83: 17 (by GC). In order to assist in the assignment of the ¾ NMR spectra of the deuterated samples, (1R, 4 R)- and (1R, 45)-dihydrocarvones of natural isotopic abundance were also prepared at high de from their parent (4R)- and (45)-carvones by reaction with an ene reductase. Here, the relevant carvone (5 mM) was shaken with 500 m% of ene reductase (JM, ENE101) in 500 /<L of non-deuterated Tris buffer (100 mM, pH 8.0) containing 2 vol.% DMSO and 10 mM NADH for 6 hours at room temperature. ² ¾0 (100 /<L) was added to the sample for field locking purposes, and the reaction mixture was analysed immediately by ¾ NMR spectroscopy.

GC-FID: Following the reactions, an aliquot of the solution was extracted with a 2 ^c volume of C ² HCl3, and then centrifuged at 18 800 ^c g for 5 minutes before being transferred to glass vials for analysis by GC-FID according to the method below. Column: DB-1701 (Agilent), 30 m length, 0.25 mm diameter, 0.25 /an film thickness; Carrier: He (CP grade), 0.5 mL minute (constant flow); Inlet temperature: 230 ^° C; Injection conditions: Splitless with split flow 60 mL/min, splitless time 0.8 mins, purge 5 mL/min.; Injection volume: 0.5 uL Detection: FID; Detector temperature: 150 °C; Detection gases: ¾ (35 mL/min), air (350 mL/min), makeup N2 (40 mL/min); Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 50 ^° C

5 25 Ramp to 250 °C at 10 °C/min

25 35 Hold at 250 °C for 10 mins

GC-MS: Following extraction and analysis by GC-FID (above) the reaction solutions were analysed by GC- MS according to the method below. Column: DB-1701 (agilent), 30 m length, 0.25 mm diameter, 0.25 on (film thickness); Carrier: He (CP grade), 100 kPa (constant pressure); Inlet temperature: 250 ^° C; Injection conditions: Split (10:1) with split flow 12 mL/min, splitless time 0.7 mins, purge 5 mL/min; Detection: Mass Spec, El (70 eV), source temperature 230 ^° C. Scan range 50 - 650 amu with a scan rate of 5 Hz. Transfer line 300 °C; Oven heating profile:

Time (minutes) Temperature

0 5 Hold at 50 ^° C

5 16.3 Ramp to 275 °C at 20 °C/min

16.3 18.8 Hold at 275 °C for 2.5 mins

H NMR spectroscopy: After removal of the catalyst, the unmodified reaction solutions were analysed by ¾ NMR spectroscopy at 500 MHz and 298 K. In order to confirm assignments, ¾-¾ correlation spectroscopy (COSY) was also conducted on the samples as required.

Results are shown in Figure 26 (reaction A) and Figure 27 (reaction B).

A: [1, 2- ² H ₂ ]-(lR, 4R)-dihydrocarvone

Analysis by GC-FID confirmed the high conversion of substrate to product, and the high selectivity for the trans-1,4 diastereomer (see Figure 26(a)). The slightly reduced diastereomeric excess (97 %) is most likely a consequence of the racemisation of the dihydrocarvone product, which occurs slowly in aqueous solutions. Quantitative analysis revealed that there was a considerable loss of product from the reaction mixture when ¾ was flowed across the headspace, and so a mass balance was not achieved in this case. Sealing the reaction under 2 bar ¾ reduced the product losses, but still only yielded a recovery of about 30 % of the theoretical quantity. The site and extent of ² H labelling was demonstrated by ¾ NMR spectroscopy (see Figure 26 (b)), the assignment of which correlated well with those of previous authors. Changes to the spectrum following the deuteration reaction confirmed both the highly specific ² H incorporation, and high diastereoselectivity that was achieved. Disappearance of the multiplet at d = 2.61 ppm (labelled b in the diagram) and collapse of the coupling on the doublet at d = 0.99 ppm with J= 6.4 Hz, were clear evidence of the ² H installation on Cl . Similarly, loss of the pseudo- quartet peak at d = 1.41 ppm (labelled C _b in the diagram), with simultaneous loss of coupling on signals representing neighbouring protons (da and db at d =

1.94 ppm and d = 1.72 ppm, respectively), provided evidence of a ² H nucleus at C2. The preservation of the peak at d = 2.18 ppm (labelled c _a in the diagram), which collapses from a multiplet to a broad singlet, is evidence that only a single ² H nucleus is installed on C2. It is likely therefore, that the two ² H nuclei are added in a trans- 1 ,2 relationship, which is in accordance with previous mechanistic studies of similar ene reductase enzymes. In this case, the ² H on C2 gives rise to an additional stereocentre, such that the product may be tentatively assigned as [1R, 2R- ² H ₂ ]-(4R)-dihydrocarvoneans-stereospecificity. Finally, GC-MS analysis of the reaction solution further confirms the addition of two ² H nuclei across the molecule, with the molecular ion being seen to shift from m/z = 152.1 for [CioHi ₆ 0 ⁺ ‘], to 154.1 for [ ² H2-CioHi40 ⁺ ‘], as shown in Figure 26 (c). B: [1, 2- ² H ₂ J-(lR, 4S)-dihydrocarvone

Analysis by GC-FID yielded results that were similar to those for Reaction A described above. Again, conversion from (45)-carvone to (1R, 45)-dihydrocarvone was found to be virtually quantitative (see Figure 27 (a)), though evaporation meant that recovery of the product was quite poor. Conducting the reaction in a sealed vial under a balloon pressure of ¾ (as opposed to a dynamic flow of ¾ across the headspace) helped to improve the product yield to around 30 % of the theoretical quantity. Unlike reaction A, the cis- (1R, 45)- isomer if formed, which represents the least stable of the two possible diastereomeric products (with racemisation giving rise to a slightly diminished de of 96 %). ³ H NMR spectroscopic analysis of the reaction solution provided insight into the extent and location of ² H incorporation into the product. Here, the dihydrocarvone standard prepared by a conventional Zn reduction was not found to be useful, as it contained mostly the thermodynamically favoured trans-1,4 dihydrocarvone isomer (see Figure 27 (a)). Instead, a standard prepared by supplying the ene reductase with (45)-carvone and a super-stoichiometric quantity of NADH in non-deuterated buffer was found to generate a suitable sample of (1R, 45)-dihydrocarvone of natural isotopic abundance for comparison. The ³ H NMR spectrum of the deuterated product is less well resolved than in Reaction A, but the disappearance of signals at d = 2.56 ppm and d = 1.58 ppm (labelled b and Cb respectively) along the collapse of coupling on the doublet at 3 = 1.05 ppm can be clearly seen (Figure 27 (b)). The convoluted peak at d = 1.93 ppm retains a relative integration of 3H on going from the standard to the deuterated reaction, confirming that the area of signal c _a is not diminished. All of these factors provide evidence for two ² H nuclei being installed across the double bond, although the likely trans- 1 ,2 arrangement cannot be confirmed unambiguously. Finally, GC-MS analysis of the reaction solution further indicates the addition of two ² H nuclei across the molecule, with the molecular ion being seen to shift from m/z = 152.1 for [CioHieCT], to 154.1 for [ ² H2-CioHi40 ^+‘ ], as shown in Figure 27 (c).

Example 10

This Example demonstrates the method of the invention in selective tritiation, wherein x = 3 for the source of the isotopic label ¾0 (i.e. ³ ¾0).

³ ¾0 from PerkinElmer ^® (500 pL, pH 8.0, diluted with ¾0 to an activity of 18.5 MBq; i.e. around 0.3 ppm ³ H in the ³ ¾0 / ¾0 mixture) containing Tris.HCl (100 mM) and NAD ⁺ (5 mM) was sealed in a conical glass flask with a Suba-Seal, and sparged with gaseous N2 and then gaseous ¾ for 30 minutes each. 5 pL of R. eutropha soluble hydrogenase (SEQ ID NOs: 1,2,3,30,31) was added, and the reaction mixture was allowed to stand at room temperature under a balloon pressure of ¾ gas for 16 hours. A UV torch (l = 360 nm) was used to confirm that NADH was been formed under these conditions.

To confirm that the formed NADH was labelled with ³ H at the 4-position, a subsequent experiment was setup with the same ³ ¾0 solution and 0.5 mM NAD ⁺ . To this second solution was added 10 mM acetophenone, 2 vol.% of DMSO and 0.5 mg of ^-selective alcohol dehydrogenase (ADH101). 5 mΐ _^ of R. eutropha soluble hydrogenase (SEQ ID NOs: 1,2,3,30,31) was added, and the reaction mixture was allowed to stand at room temperature under a balloon pressure of H2 gas for 16 hours. The (R)-phenylethanol product was extracted into 1 mL of C ² HCl3, and dried with 150 mg of anhydrous P2O5 to remove residual H2O.

Product analysis was conducted by ³ H NMR spectroscopy in the manner detailed above, and confirmed a conversion of > 80 % to the 1-phenylethanol product (see Figure 28A). The absolute concentration of extracted 1-phenylethanol was determined by reference to the residual CHCI3 signal (S = 7.26 ppm). The ³ H NMR spectra shown in Figure 28A were generated with the following parameters: 500 MHz, 256 scans, LB = 0.3 Hz, C ² HC1 ₃ , 298 K.

To establish the extent of ³ H radiolabelling on the product, liquid scintillation counting (LSC) of the C ² HCl3 extract was conducted as follows: LSC was carried out on a Beckman LS6500 machine, using 500 må of analyte solution and 5 mL of PerkinElmer ^® Ultima Gold LLT scintillant. A calibration was conducted to establish the LSC response for a known quantity of ³ H using measured amounts of [ ³ H]-toluene

(PerkinElmer ^® LSC standard, 43.3 kBq/g) dissolved in 500 uL of C ² HCl3 _. A counting time of 1 minute was used at each concentration, and an exemplar plot is shown in Figure 28B. From the LSC calibration, the radioactivity of the extracted product sample was determined to be 12 Bq. From the ³ H NMR spectrum it was possible to determine the quantity of H2O (and hence, ³ ¾0) carried over from the aqueous phase, and so subtract this from the calculated radioactivity of the product. Hence, it was determined that the product ( R )- phenylethanol had an activity of 32 MBq/mol, indicating a ³ H incorporation of around 30 ppb.

This experiment thus confirms that H2-driven NADH recycling may be driven in ³ ¾0 to deliver a [ ³ H]- labelled product.

Aspects of the invention

1. A method of producing a reduced labelled cofactor comprising one or more Ή atom, wherein x is 2 or 3, wherein said method comprises:

i) providing a composition comprising (i) Ή ⁺ ions and (ii) an oxidised cofactor;

ii) transferring electrons from an electron source to a first polypeptide which is an

NADH:acceptor oxidoreductase or an NADPH:acceptor oxidoreductase or a functional derivative or fragment thereof; and

iii) contacting the Ή ⁺ ions and the oxidised cofactor with the first polypeptide thereby

reducing the oxidised cofactor to form a reduced labelled cofactor comprising one or more XH atoms. 2. A method according to aspect 1, wherein said method is a method of producing a reduced labelled reaction product comprising one or more Ή atom, wherein x is 2 or 3, wherein said method comprises producing a reduced labelled cofactor according to aspect 1 ; and

iv) contacting the reduced labelled cofactor and an oxidised reactant with at least one enzyme that is an NADH-dependent oxidoreductase or an NADPH-dependent oxidoreductase or a functional derivative or fragment thereof such that the enzyme selectively transfers an Ή atom from the reduced labelled cofactor to the oxidised reactant thereby producing a reduced labelled reaction product and an oxidised cofactor.

3. A method according to aspect 2 which further comprises reducing the oxidised cofactor produced in step (iv) of aspect 2 in a method according to aspect 1.

4. A method according to aspect 2 which comprises producing a reduced labelled reaction product according to steps (i) to (iv) of aspects 1 and 2, and repeating steps (ii) to (iv) multiple times, thereby recycling the cofactor.

5. A method according to any one of the preceding aspects wherein the Ή ⁺ ions are provided as ² H ₂ 0 or ³ H ₂ 0.

6. A method according to any one of the preceding aspects wherein:

(i) the oxidised cofactor is NAD ⁺ , NADP ⁺ , or a labelled version of NAD ⁺ or NADP ⁺ comprising at least one Ή atom, wherein preferably reducing the oxidised cofactor to form a reduced labelled cofactor comprises adding an Ή atom at the 4- position of the nicotinamide ring of the oxidised cofactor; and/or

(ii) the Ή ⁺ ions are transferred directly from the composition comprising Ή ⁺ ions to the first polypeptide.

7. A method according to any one of the preceding aspects wherein the first polypeptide transfers an *H- anion to the oxidised cofactor thereby forming the reduced labelled cofactor, wherein preferably:

A. the first polypeptide comprises a flavin group; and/or

B. the first polypeptide has a structure comprising a Rossmann fold; and/or

C. the first polypeptide comprises or consists of a diaphorase moiety; and/or

D. the first polypeptide consists or comprises of one or more than one of: i) the amino acid sequence of Ralstonia eutropha diaphorase HoxF (SEQ ID NO: 1) or an amino acid sequence having at least 60% homology therewith;

ii) the amino acid sequence of Ralstonia eutropha diaphorase HoxU (SEQ ID NO: 2) or an amino acid sequence having at least 60% homology therewith;

iii) the amino acid sequence of Ralstonia eutropha diaphorase Hoxl (SEQ ID NO: 3) or an amino acid sequence having at least 60% homology therewith;

iv) the amino acid sequence of the 51 kDa protein of the flavoprotein (Fp) subcomplex of Complex I of Bos taurus (SEQ ID NO: 4) or an amino acid sequence having at least 60% homology therewith;

v) the amino acid sequence of the 24kDa subcomplex of Complex I of Bos taurus (SEQ ID NO: 5) or an amino acid sequence having at least 60% homology therewith;

vi) the amino acid sequence of Ralstonia eutropha NAD ⁺ -dependent formate dehydrogenase diaphorase moiety FdsB (SEQ ID NO: 6) or an amino acid sequence having at least 60% homology therewith;

vii) the amino acid sequence of Ralstonia eutropha NAD ⁺ -dependent formate dehydrogenase diaphorase moiety FdsG (SEQ ID NO: 7) or an amino acid sequence having at least 60% homology therewith;

viii) the amino acid sequence of Rhodobacter capsulatus NAD ⁺ -dependent formate dehydrogenase, diaphorase moiety FdsB (SEQ ID NO: 8) or an amino acid sequence having at least 60% homology therewith;

ix) the amino acid sequence of Rhodobacter capsulatus NAD ⁺ -dependent formate dehydrogenase, diaphorase moiety FdsG (SEQ ID NO: 9) or an amino acid sequence having at least 60% homology therewith;

x) the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase I gamma subunit (SEQ ID NO: 10) or an amino acid sequence having at least 60% homology therewith;

xi) the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase I beta subunit (SEQ ID NO: 11) or an amino acid sequence having at least 60% homology therewith;

xii) the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase II gamma subunit (SEQ ID NO: 12) or an amino acid sequence having at least 60% homology therewith;

xiii) the amino acid sequence of the amino acid sequence of the NADPH oxidoreductase moiety from Pyrococcus furiosus soluble hydrogenase II beta subunit (SEQ ID NO: 13) or an amino acid sequence having at least 60% homology therewith;

xiv) the amino acid sequence of the diaphorase moiety of Rhodococcus opacus soluble hydrogenase HoxF (SEQ ID NO: 14) or an amino acid sequence having at least 60% homology therewith; xv) the amino acid sequence of the diaphorase moiety of Rhodococcus opacus soluble hydrogenase HoxU (SEQ ID NO: 15) or an amino acid sequence having at least 60% homology therewith; xvi) the amino acid sequence of the diaphorase moiety of Allochromatium vinosum soluble

hydrogenase HoxF (SEQ ID NO: 16) or an amino acid sequence having at least 60% homology therewith;

xvii) the amino acid sequence of the diaphorase moiety of Allochromatium vinosum soluble

hydrogenase HoxU (SEQ ID NO: 17) or an amino acid sequence having at least 60% homology therewith;

xviii) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina HoxlF (SEQ ID NO: 18) or an amino acid sequence having at least 60% homology therewith;

xix) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina soluble

hydrogenase HoxlU (SEQ ID NO: 19) or an amino acid sequence having at least 60% homology therewith;

xx) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina Hox2F (SEQ ID NO: 20) or an amino acid sequence having at least 60% homology therewith;

xxi) the amino acid sequence of the diaphorase moiety of Thiocapsa roseopersicina soluble

hydrogenase Hox2U (SEQ ID NO: 21) or an amino acid sequence having at least 60% homology therewith;

xxii) the amino acid sequence of the diaphorase moiety of Synechocystis sp. PCC 6803 HoxF (SEQ ID NO: 22) or an amino acid sequence having at least 60% homology therewith;

xxiii) the amino acid sequence of the diaphorase moiety of Synechocystis sp. PCC 6803 HoxU (SEQ ID NO: 23) or an amino acid sequence having at least 60% homology therewith;

xxiv) the amino acid sequence of the diaphorase moiety of Synechococcus elongatus PCC 6301 HoxF (SEQ ID NO: 24) or an amino acid sequence having at least 60% homology therewith;

xxv) the amino acid sequence of the diaphorase moiety of Synechococcus elongatus PCC 6301 HoxU (SEQ ID NO: 25) or an amino acid sequence having at least 60% homology therewith; xxvi) the amino acid sequence of Hydrogenophilus thermoluteolus diaphorase HoxF (SEQ ID NO:

26) or an amino acid sequence having at least 60% homology therewith;

xxvii) the amino acid sequence of Hydrogenophilus thermoluteolus diaphorase HoxU (SEQ ID NO:

27) or an amino acid sequence having at least 60% homology therewith;

xxviii) the amino acid sequence of Chlamydomonas reinhardtii Ferredoxin-NADP+ reductase (SEQ ID NO: 28) or an amino acid sequence having at least 60% homology therewith;

xxix) the amino acid sequence of Anabaena Ferredoxin-NADP+ reductase (SEQ ID NO: 29) or an amino acid sequence having at least 60% homology therewith;

xxx) the amino acid sequence of Ralstonia eutropha diaphorase HoxF (SEQ ID NO: 70) or an amino acid sequence having at least 60% homology therewith; xxxi) the amino acid sequence of Ralstonia eutropha diaphorase with inactive hydrogenase (SEQ ID NO: 1 and/or 2 and/or 69 and/or 31) or an amino acid sequence having at least 60% homology therewith or a functional fragment, derivative or variant thereof; wherein more preferably the first polypeptide consists or comprises of the Ralstonia eutropha NAD ⁺ -reducing soluble hydrogenase or a functional fragment, derivative or variant thereof.

8. A method according to any one of the preceding aspects wherein the electron source comprises a second polypeptide which is an oxidising enzyme or functional derivative or fragment thereof capable of oxidising a reductant to extract electrons, wherein the second polypeptide transfers electrons from the reductant to the first polypeptide via an electronically-conducting pathway, wherein preferably (i) electrons are directly transferred along the electronically-conducting pathway or (ii) electron transfer along the electronically-conducting pathway is mediated by one or more electron mediators; wherein more preferably:

A. the first polypeptide and the second polypeptide constitute component parts of a modular, multidomain or multicomponent protein or protein complex; and/or

B. the second polypeptide is selected or modified to oxidise ¾ or ¾ under the conditions of the method; and/or

C. the second polypeptide is a hydrogenase enzyme or a functional derivative or fragment thereof, wherein preferably the hydrogenase is selected from i) the amino acid sequence of Ralstonia eutropha soluble hydrogenase moiety (SEQ ID NOs: 30 and/or 31) or an amino acid sequence having at least 60% homology therewith; ii) the amino acid sequence of Ralstonia eutropha membrane-bound hydrogenase moiety (SEQ ID NOs: 32 and/or 33 and/or 34) or an amino acid sequence having at least 60% homology therewith;

iii) the amino acid sequence of Ralstonia eutropha regulatory hydrogenase moiety (SEQ ID NOs:

35 and/or 36) or an amino acid sequence having at least 60% homology therewith; iv) the amino acid sequence of Escherichia coli hydrogenase 1 (SEQ ID NOs:37 and/or 38) or an amino acid sequence having at least 60% homology therewith;

v) the amino acid sequence of Escherichia coli hydrogenase 2 (SEQ ID NOs:39 and/or 40) or an amino acid sequence having at least 60% homology therewith;

vi) the amino acid sequence of Aquifex aeolicus hydrogenase 1 (SEQ ID NO:41 and/or 42) or an amino acid sequence having at least 60% homology therewith; vii) the amino acid sequence of Hydrogenovibrio marinus hydrogenase (SEQ ID NOs: 43 and/or 44) or an amino acid sequence having at least 60% homology therewith;

viii) the amino acid sequence of Thiocapsa roseopersicina hydrogenase (SEQ ID NOs: 45 and 46) or an amino acid sequence having at least 60% homology therewith;

ix) the amino acid sequence of Alteromonas macleodii hydrogenase (SEQ ID NOs: 47 and/or 48) or an amino acid sequence having at least 60% homology therewith;

x) the amino acid sequence of Rhodococcus opacus soluble hydrogenase moiety (SEQ ID NOs: 49 and/or 50) or an amino acid sequence having at least 60% homology therewith;

xi) the amino acid sequence of Allochromatium vinosum membrane bound hydrogenase (SEQ ID NOs: 51 and/ or 52) or an amino acid sequence having at least 60% homology therewith; xii) the amino acid sequence of Desulfovibrio fructosovorans membrane bound hydrogenase (SEQ ID NOs: 53 and/ or 54) or an amino acid sequence having at least 60% homology therewith; xiii) the amino acid sequence of Clostridium pasteurianum iron-iron hydrogenase (SEQ ID NOs: 55) or an amino acid sequence having at least 60% homology therewith;

xiv) the amino acid sequence of Clostridium acetobutylicum iron-iron hydrogenase (SEQ ID NOs:

56) or an amino acid sequence having at least 60% homology therewith;

xv) the amino acid sequence of Chlamydomonas reinhardtii iron-iron hydrogenase (SEQ ID NOs:

57) or an amino acid sequence having at least 60% homology therewith;

xvi) the amino acid sequence of Desulfomicrobium baculatum nickel-iron selenium hydrogenase (SEQ ID NOs: 58 and/ or 59) or an amino acid sequence having at least 60% homology therewith;

xvii) the amino acid sequence of Hydrogenophilus thermoluteolus soluble hydrogenase moiety (SEQ ID NOs: 60 and/or 61) or an amino acid sequence having at least 60% homology therewith; xviii) the amino acid sequence of Desulfovibrio vulgaris Nickel Iron hydrogenase (pdb 1H2A) (SEQ ID NOs: 62 and/ or 63) or an amino acid sequence having at least 60% homology therewith; xix) the amino acid sequence of Desulfovibrio gigas Periplasmic [NiFe] hydrogenase (SEQ ID NOs:

64 and/or 65) or an amino acid sequence having at least 60% homology therewith;

xx) the amino acid sequence of Salmonella enterica serovar Typhimurium LT2 nickel-iron

hydrogenase 5 (SEQ ID NO: 66 and/or 67) or an amino acid sequence having at least 60% homology therewith.

xxi) the amino acid sequence of Pyrococcus furiosus soluble alpha subunit (SEQ ID NOs: 68) or an amino acid sequence having at least 60% homology therewith; or a functional fragment, derivative or variant thereof. A method according to any one of aspects 1 to 7 wherein

i) the electron source comprises a synthetic organic, inorganic or metallic oxidation catalyst capable of oxidising a reductant to extract electrons, wherein the oxidation catalyst transfers electrons from the reductant to the first polypeptide via an electronically- conducting pathway; wherein preferably the oxidation catalyst comprises platinum, palladium, iridium nickel, rhodium and/or ruthenium; or

ii) the electron source comprises an electrode connected to an electrode controller, wherein the electrode is connected to the first polypeptide via an electronically-conducting pathway.

10. A method according to aspects 8 or 9 wherein the reductant oxidised by the second polypeptide or the oxidation catalyst is ¾ or *¾, preferably ¾.

11. A method according to any one of aspects 8 to 10 wherein the electron source comprises a second polypeptide as defined in aspect 8 or an oxidation catalyst as defined in aspect 9, and wherein the electron source and the first polypeptide are each in electronic contact with an electronically conducting support, wherein preferably: a. the electron source and the first polypeptide are each in electronic contact with the same electronically conducting support, wherein preferably the support is an electronically conducting particle; or b. the electron source is in electronic contact with an electronically conducting first support and the first polypeptide is in electronic contact with an electronically conducting second support; and the first support is in electronic contact with the second support.

12. A method according to aspect 11 wherein the or each support comprises a material comprising carbon, a metal or metal alloy, a metal oxide or mixed metal oxide, a metal hydroxide, a metal chalcogenide, a semi-conducting material, or an electronically-conductive polymer, or mixtures thereof; or according to aspect 9 wherein the electron source comprises an electrode connected to an electrode controller and the electrode comprises a material comprising carbon, a metal or metal alloy, a metal oxide or mixed metal oxide, a metal hydroxide, a metal chalcogenide, or an electronically-conductive polymer, or mixtures thereof;

wherein preferably the material comprises:

i) Carbon, preferably graphite, carbon nanotube(s), carbon black, activated carbon, carbon nanopowder, vitreous carbon, carbon fibre(s), carbon cloth, carbon felt, carbon paper, graphene, highly oriented pyrolytic graphite, pyrolytic graphite, or doped diamond; and/or ii) a metal or metal alloy selected from gold, silver, tungsten, iridium, platinum, palladium, copper, titanium, brass, and steel; and/or

iii) a material selected from titanium oxide, indium oxide, tin oxide and indium tin oxide; A method according to any one of aspects 2 to 12 wherein the at least one enzyme that is an NADH- dependent oxidoreductase or NADPH-dependent oxidoreductase is at least one of an NAD(P)H- dependent alcohol dehydrogenase, an NAD(P)H-dependent ene reductase, an NAD(P)H-dependent imine reductase or an NAD(P)H-dependent amino-acid dehydrogenase, wherein preferably the at least one enzyme that is an NADH-dependent oxidoreductase or NADPH-dependent oxidoreductase is at least one of an alcohol dehydrogenase or an amino acid dehydrogenase. A system for performing a method according to any one of aspects 1 to 13, the system comprising: i) a composition comprising (i) Ή ⁺ ions wherein x is 2 or 3 and (ii) an oxidised cofactor, wherein preferably the composition is as defined in aspect 5 and/or the oxidised cofactor is as defined in aspect 6;

ii) an electron source, wherein preferably the electron source is as defined in any one of aspects 8 to 12; and

iii) a first polypeptide which is an NADH: acceptor oxidoreductase or an NADPH: acceptor oxidoreductase or a functional derivative or fragment thereof, wherein preferably the first polypeptide is as defined in any one of aspects 7;

wherein the system is configured such that, in use, (a) electrons are transferred from the electron source to the first polypeptide and (b) Ή ⁺ ions and the oxidised cofactor are contacted with the first polypeptide so as to reduce the oxidised cofactor to form a reduced labelled cofactor comprising one or more Ή atoms. A method for producing an oxidised labelled cofactor comprising one or more Ή atom, wherein x is 2 or 3, comprising producing a reduced labelled cofactor comprising one or more Ή atom according to any one of aspects 1 to 13; and oxidising the reduced labelled cofactor.