α,β-Unsaturated aldehydes are widely used in the organic synthesis of fine chemicals for application in products such as flavoring agents, fragrances and pharmaceuticals. In the selective oxidation of α,β-unsaturated alcohols to the corresponding α,β-unsaturated aldehydes, it remains challenging to overcome poor selectivity, overoxidation and a low atom efficiency in chemical routes.
An E. coli strain coexpressing the NADP+-specific alcohol dehydrogenase YsADH and the oxygen-dependent NADPH oxidase TkNOX was constructed; these components enabled the NADP+ regeneration and catalyzed the oxidation of 100 mM 3-methyl-2-buten-1-ol to 3-methyl-2-butenal with a yield of 21.3%. The oxygen supply was strengthened by introducing the hemoglobin protein VsHGB into recombinant E. coli cells and replacing the atmosphere of the reactor with pure oxygen, which increased the yield to 51.3%. To further improve catalytic performance, the E. coli cells expressing the multifunctional fusion enzyme YsADH-(GSG)-TkNOX-(GSG)-VsHGB were generated, which completely converted 250 mM 3-methyl-2-buten-1-ol to 3-methyl-2-butenal after 8 h of whole-cell oxidation. The reaction conditions for the cascade biocatalysis were optimized, in which supplementation with 0.2 mM FAD and 0.4 mM NADP+ was essential for maintaining high catalytic activity. Finally, the established whole-cell system could serve as a platform for the synthesis of valuable α,β-unsaturated aldehydes through the selective oxidation of various α,β-unsaturated alcohols.
The construction of a strain expressing the fusion enzyme YsADH-(GSG)-TkNOX-(GSG)-VsHGB achieved efficient NADP+ regeneration and the selective oxidation of various α,β-unsaturated alcohols to the corresponding α,β-unsaturated aldehydes. Among the available redox enzymes, the fusion enzyme YsADH-(GSG)-TkNOX-(GSG)-VsHGB has become the most recent successful example to improve catalytic performance in comparison with its separate components.
α,β-Unsaturated aldehydes serve as important intermediates in the organic synthesis of an extended range of fine chemicals for use in products such as flavoring agents, fragrances and pharmaceuticals [1,2,3]. For example, citral (3,7-dimethyl-2,6-octadien-1-al) is in high demand for the production of ionones, vitamins A and E, and carotenoids . α,β-Unsaturated aldehydes can be obtained through the selective oxidation of the corresponding α,β-unsaturated alcohols via either chemical catalysis or biocatalysis [3, 5,6,7]. Traditional chemical oxidation methods have required the use of equimolar amounts of oxidizing reagents, whose atom efficiency is relatively low. Moreover, the practical application of chemical routes is often limited by overoxidation, poor selectivity and the use of organic solvents and toxic compounds . Alternatively, biocatalytic oxidation has raised great interest because of its excellent selectivity and environmentally friendly nature as well as the mild reaction conditions involved [9,10,11].
Both alcohol oxidases and alcohol dehydrogenases are attractive biocatalysts used for the selective oxidation of α,β-unsaturated alcohols. Alcohol oxidases utilize the cheap mild oxidant molecular oxygen and generally form highly reactive hydrogen peroxide as a byproduct . In most cases, the toxicity of hydrogen peroxide can be partially avoided by the catalytic dismutation of H2O2 into O2 and water using catalase. A prominent example is the recombinant aryl alcohol oxidase from Pleurotus eryngii used for the selective oxidation of trans-2-hexen-1-ol to trans-2-hexenal, in which the turnover number exceeds 2.2 million . The enzyme in its active form is obtained from inclusion bodies in a cell extract, which prevents the use of whole-cell biotransformation . Compared with isolated enzymes, the use of whole-cell catalysts simplifies the procedure, reduces costs and improves the enzyme stability. Despite great potential, the number of characterized alcohol oxidases is very limited, in contrast to the wide array of alcohol dehydrogenases with various substrate specificities [7, 13,14,15,16]. Alcohol dehydrogenases catalyze reversible oxidation reactions and require NAD(P)+, suggesting that efficient NAD(P)+ regeneration is needed to shift the reaction equilibrium toward product formation [11, 17].
NAD(P)+ regeneration can be substrate-coupled or enzyme-coupled, where the latter does not require the use of excess cosubstrate to ensure the efficient oxidation . Among enzyme-coupled approaches, the cascade biotransformation of alcohol dehydrogenase and NAD(P)H oxidase is much more atomically efficient for NAD(P)+ recycling, where the direct oxidation of NAD(P)H by molecular oxygen forms hydrogen peroxide or water . In particular, water-forming NAD(P)H oxidase is ideal because there are no byproducts [19, 20]. In multiple enzymatic cascade reactions, the possibilities and advantages of enzyme fusions have been explored for various enzyme types, including fusions of redox enzymes [21,22,23,24,25,26]. Through this approach, enzymes can be produced simultaneously and are colocalized in cells. The fusion of ADH with NOX to perform alcohol oxidation supported the rapid regeneration of NADP+, and the cascade reaction was more efficient than the separate enzymes .
Our previous work showed that NADP+-specific YsADH, an α,β-unsaturated alcohol dehydrogenase from Yokenella sp. WZY002, exhibited high activity and stability in the selective oxidation of crotonyl alcohol to crotyonyl aldehyde . In this work, the selective oxidation of 3-methyl-2-buten-1-ol to 3-methyl-2-butenal was chosen as the model reaction, considering that both 3-methyl-2-buten-1-ol and 3-methyl-2-butenal serve as important organic synthesis intermediates. The use of the NADPH oxidase TkNOX together with VsHGB hemoglobin, capable of binding and releasing oxygen, was explored for the regeneration of NADP+ and the improvement of catalytic efficiency of selective oxidation [28,29,30] (Scheme 1). Moreover, the fusion protein of YsADH-(linker)-TkNOX-(linker)-VsHGB was constructed to increase the catalytic performance, resulting in the efficient whole-cell oxidation of various α,β-unsaturated alcohols to the corresponding α,β-unsaturated aldehydes.
Results and discussion
Cascade catalysis of alcohol dehydrogenase, NADPH oxidase and hemoglobin
Alcohol dehydrogenase from Yokenella sp. WZY002 is highly active in the oxidation of various α,β-unsaturated alcohols to the corresponding α,β-unsaturated aldehydes . To be compatible with YsADH activity (e.g., temperature and pH optima), a thermostable NADPH oxidase from Thermococcus kodakaraensis was chosen to catalyze the oxidation of NADPH, predominantly converting O2 to H2O . A recombinant strain expressing YsADH alone and a strain coexpressing YsADH and TkNOX were successfully constructed and induced, and the formation of inclusion bodies was not observed in these strains (Fig. 1, Additional file 1: Figure S1). It was noted that the cooccurrence of YsADH and TkNOX significantly affected the expression level of YsADH. In particular, the activity of YsADH was reduced from 3568 U/g (expression of YsADH alone) to 650 U/g (coexpression of YsADH and TkNOX) (Additional file 1: Table S1). The whole-cell catalyst expressing YsADH alone catalyzed the oxidation of 100 mM 3-methyl-2-buten-1-ol to 3-methyl-2-butenal with a yield of 11.75% (Table 1). The yield of 3-methyl-2-butenal was increased up to 21.3% when cells coexpressing YsADH and TkNOX were used as biocatalysts, indicating that alcohol oxidation benefited from the NADP+ regeneration.
Whole-cell oxidation catalyzed by oxygen-dependent enzymes might be restricted by the oxygen supply because of the limited solubility of oxygen in water . To improve the supply of oxygen, the gene encoding hemoglobin from Vitreoscilla stercoraria was further introduced into the recombinant cells coexpressing YsADH and TkNOX, giving rise to a strain coexpressing YsADH, TkNOX and VsHGB . Cell-free extracts of the cells coexpressing YsADH, TkNOX and VsHGB were prepared, and the activities of YsADH and TkNOX were determined to be 613 U/g and 1542 U/g, respectively. The use of the strain coexpressing YsADH, TkNOX and VsHGB increased the yield of 3-methyl-2-butenal to 35.48%. In addition, the atmosphere of the reactor was replaced with pure oxygen to increase the supply of oxygen, in which the yield of 3-methyl-2-butenal reached 51.3% (Table 1). To determine whether overoxidation of the product occurred, the possible side products isovaleraldehyde, isovaleric acid and 3,3-dimethylacrylic acid were verified by gas chromatography. The results indicated that none of these products were detectable, demonstrating that the reaction conditions were mild enough for the oxidation of 3-methyl-2-buten-1-ol to 3-methyl-2-butenal.
Construction of YsADH/TkNOX/VsHGB fusion proteins and their catalytic performance
In redox reactions, enzyme fusions have been approved as an efficient approach to support the rapid regeneration of NADP+ . To test whether the fusion of YsADH and TkNOX could improve the selective oxidation of 3-methyl-2-buten-1-ol, a YsADH-TkNOX fusion with a GGGGS linker was initially constructed and successfully induced (Fig. 2). Whole-cell catalysis in cells expressing YsADH-(GGGGS)-TkNOX indicated that the yield of 3-methyl-2-butenal was significantly increased from 51.3% to 80.57% (Fig. 3). It was suggested that the length of the flexible linkers might affect the activity of the fusion proteins . Then, fusion genes were constructed and compared by linking the YsADH and TkNOX with GGGGS as well as other peptide linkers ((GGGGS)2, GSG and (GSG)2). All four resulting fusion genes were transformed into E. coli and then induced, and the formation of inclusion bodies was not observed in these strains (Fig. 2, Additional file 1: Figure S2). In contrast to the strain coexpressing the individual enzymes, all of the fusion proteins exhibited much higher catalytic efficiency (Fig. 3). The fusion enzymes with the GSG, (GSG)2 or GGGGS linker showed similar activity against the substrate 3-methyl-2-buten-1-ol, which was higher than that of the enzyme with the (GGGGS)2 linker. The GSG linker was finally used to generate cells expressing the fusion protein YsADH-(GSG)-TkNOX-(GSG)-VsHGB or VsHGB-(GSG)-TkNOX-(GSG)-YsADH (Additional file 1: Figure S3), and both of these fusions completely converted 100 mM 3-methyl-2-buten-1-ol to 3-methyl-2-butenal after 2 h of whole-cell oxidation. The functional expression of both the YsADH and TkNOX enzymes was also verified by measuring their activities in cell-free extracts comprising YsADH-(GSG)-TkNOX-(GSG)-VsHGB or VsHGB-(GSG)-TkNOX-(GSG)-YsADH. The specific activities of YsADH and TkNOX in the cell-free extracts comprising YsADH-(GSG)-TkNOX-(GSG)-VsHGB were determined to be 801 U/g and 983 U/g, respectively, while those in the cell-free extract comprising VsHGB-(GSG)-TkNOX-(GSG)-YsADH were 752 U/g and 1064 U/g, respectively (Additional file 1: Table S1). In the previous case involving the fusions of alcohol dehydrogenase with cyclohexanone monooxygenase, the fusion protein with the order alcohol dehydrogenase-cyclohexanone monooxygenase showed low to no alcohol dehydrogenase activity . The fusion proteins in which the components were ordered YsADH-(GSG)-TkNOX-(GSG)-VsHGB and VsHGB-(GSG)-TkNOX-(GSG)-YsADH not only maintained high levels of both YsADH and TkNOX activities, but the ratio of YsADH and TkNOX activities was also more optimal than that in the cells coexpressing YsADH, TkNOX and VsHGB separately.
Evaluation of factors affecting the catalytic efficiency of whole-cell catalysts expressing YsADH-(GSG)-TkNOX-(GSG)-VsHGB
During whole-cell cascade biocatalysis, multiple reactions are run in the same pot, and each reaction often does not reach the optimal conditions . To achieve optimal catalytic efficiency, it is essential to orchestrate the catalytic performance of YsADH, TkNOX and VsHGB in the YsADH-(GSG)-TkNOX-(GSG)-VsHGB fusion protein. Hence, various factors, such as temperature, pH, rotation, FAD and NADP+ concentrations and the substrate concentration, were investigated when the cells comprising YsADH-(GSG)-TkNOX-(GSG)-VsHGB were chosen as whole-cell catalysts. To magnify the differences in catalytic performances, the biocatalyst loading was reduced to 0.1 g lyophilized cells in a 5 ml reaction mixture. The influence of the reaction temperature was determined over a range of 40–65 °C, and the highest yield of 3-methyl-2-butenal (70.35%) was observed at 45 °C (Fig. 4). When the temperature was greater than 45 °C, the product yield decreased as the temperature rose. Since TkNOX is highly thermostable and thermoactive, the thermal optimum might mainly correspond to that of YsADH [7, 29]. To determine the optimal pH, the reaction was carried out at pH levels ranging from 6.0 to 9.5 at 45 °C. The highest production was detected at pH 8.0 (Fig. 5), which was consistent with the pH optima of both YsADH and TkNOX [7, 29]. Similarly, rotation was optimized to be 600 rpm (Fig. 6), considering both mass transfer and shear force. It has been suggested that the expression of FAD-dependent NOXs in E. coli might result in poor activity due to the absence of FAD . The yield of 3-methyl-2-butenal (53.1%) in the presence of 0.2 mM exogenous FAD was 6.56 times higher than that without the addition of exogenous FAD. When the FAD concentration was set as 0.2 mM, 0.4 mM NADP+ was sufficient for maintaining high activity in the oxidation of 3-methyl-2-buten-1-ol (Fig. 7). When the substrate concentration was increased in a stepwise manner, typical time courses under biocatalyst loading of 0.3 g lyophilized cells in a 5 ml reaction mixture are shown in Fig. 8. The times required to completely convert 50, 100, 150, 200 and 250 mM 3-methyl-2-buten-1-ol to 3-methyl-2-butenal were 1.5, 2, 4, 6 and 8 h, respectively. A further increase in the substrate concentration to 300 mM resulted in an 80.1% yield of 3-methyl-2-butenal within 12 h, and the decrease in catalytic efficiency might be attributed to cell disintegration from the accumulation of hydrophobic compounds and/or the enzyme inactivation .
Oxidation of various α,β-unsaturated alcohols to α,β-unsaturated aldehydes
To expand the applicability of the established whole-cell oxidation, the use of various α,β-unsaturated alcohols to produce α,β-unsaturated aldehydes, some of which are of great industrial interest, were examined (Table 2). For example, retinol oxidation was performed to form retinal, which might be further converted to carotene . The oxidation of farnesol to farnesal is a key step in the synthesis of vitamin E using farnesol as starting material [35, 36]. Similar to the case of 3-methyl-2-buten-1-ol, 200 mM crotyl alcohol was completely converted to crotonaldehyde after 6 h of oxidation. The yield of crotonaldehyde (96.70%, 8 h) in the initial presence of 300 mM crotyl alcohol was even greater than that (80.1%, 12 h) in the initial presence of 300 mM 3-methyl-2-buten-1-ol. The oxidation of trans-2-hexenol, geraniol and nerol for 8 h resulted in similar catalytic performances (83.35–93.46% yields), whereas that of cinnamyl alcohol resulted in a relatively lower yield of cinnamyl aldehyde (47.49%). The results suggested that the catalytic efficiency might be associated with the solubility and/or molecule size of the substrate. In addition, enzyme inactivation through covalent modification could not be ignored since the carbonyl group of α,β-unsaturated aldehydes (e.g., crotonaldehyde) can form a Schiff base with the lysine side chain, and the cysteine thiol group of the enzyme then attacks the Cβ atom of the C=C band of α,β-unsaturated aldehydes . Efforts aimed at protein engineering with the goal of mitigating activity inhibition are currently underway in our laboratory.
As an alternative to the use of alcohol oxidase and catalase, this study developed a method for the whole-cell oxidation of α,β-unsaturated alcohols to α,β-unsaturated aldehydes based on the combination of YsADH alcohol dehydrogenase and TkNOX NADPH oxidase. Both NADP+-dependent YsADH and oxygen-dependent TkNOX were highly active and compatible with temperature and pH optima. The catalytic efficiency and the NADP+ regeneration achieved during the whole-cell oxidation were enhanced through the improvement of the oxygen supply, the overexpression of YsADH, TkNOX and VsHGB fusion proteins, and the optimization of reaction conditions. In the case of 3-methyl-2-buten-1-ol oxidation, the whole-cell cascade catalysis system enabled efficient alcohol oxidation but also overcame the poor selectivity and over oxidation that occur frequently in chemical synthesis. The established whole-cell system could be tuned to achieve the synthesis of various α,β-unsaturated aldehydes from the selective oxidation of α,β-unsaturated alcohols.
Chemicals, enzymes, plasmids and strains
The standards α,β-unsaturated alcohols and aldehydes were obtained from Sigma-Aldrich (Shanghai) Trading Co., Ltd. (Shanghai, China). Other chemicals of analytical grade were purchased from Sangon Biotech Co. Ltd (Shanghai, China) or Shanghai Jingchun Reagent Co., Ltd (Shanghai, China). The kits and the enzymes for gene manipulation were obtained from Takara Biomedical Technology Co., Ltd. (Beijing, China). The pET28a and pACYCDuet-1 vectors were used for the over-expression of the enzymes, and the E. coli strain BL21(DE3) was used as the host. E. coli cultures were grown routinely in LB medium at 37 °C for 12 h.
Cloning and overexpression of YsADH, TkNOX and VsHGB in E. coli cells
The DNA sequences encoding YsADH (GenBank accession number: KF887947), TkNOX (BAD85488) and VsHGB (AAA27584) were codon-optimized and synthesized at Vazyme Biotech Co., Ltd (Nanjing, China) (Additional file 1: Figure S4). The gene encoding YsADH was introduced into the sites NcoI/HindIII of the vector pACYCDuet-1, yielding the recombinant plasmid pACYCDuet-1-YsADH. Moreover, the gene encoding TkNOX was further inserted into the sites NdeI/XhoI of the plasmid pACYCDuet-1-YsADH, yielding the recombinant plasmid pACYCDuet-1-YsADH-TkNOX. In addition, the gene encoding VsHGB was introduced into the sites EcoRI and HindIII of the vector pET28a, offering the recombinant plasmid pET28a-VsHGB.
The recombinant plasmids pACYCDuet-1-YsADH and pACYCDuet-1-YsADH-TkNOX were transformed into the host strain E. coli BL21(DE3), giving rise to the recombiant strains E. coli BL21(DE3)/pACYCDuet-1-YsADH and E. coli BL21(DE3)/pACYCDuet-1-YsADH-TkNOX, respectively. Furthermore, the recombinant plasmid pET28a-VsHGB was transformed into the strain E. coli BL21(DE3)/pACYCDuet-1-YsADH-TkNOX, leading to the strain E. coli BL21(DE3)/pACYCDuet-1-YsADH-TkNOX/pET28a-VsHGB.
The recombinant E. coli strains were routinely grown in LB medium containing 50 μg/ml chloramphenicol and/or 50 μg/ml kanamycin at 37 °C until the OD600 of 0.6–0.8. Specifically, chloramphenicol was used for the cells containing the vector pACYCDuet-1, kanamycin was used for cells containing the vector pET28a, meanwhile both chloramphenicol and kanamycin were supplemented for cells containing both pACYCDuet-1 and pET28a vectors. Strains were induced by adding 0.3 mM IPTG and cultured at 20 °C for 12 h. Cells were washed twice using 50 mM Tris-HCl buffer (pH 8.0) and then harvested by 8000 g centrifugation at 4 °C for 10 min. Finally, lyophilized cells were obtained by freeze-drying and stored at − 20 °C for further use.
Construction and overexpression of the YsADH-(linker)-TkNOX and YsADH-(linker)-TkNOX-(linker)-VsHGB fusion enzymes in E. coli cells
The fusion genes encoding YsADH, TkNOX and VsHGB were constructed by multiple overlap extension PCR . To assembly four YsADH-(linker)-TkNOX fusion genes, the stop codon of the YsADH gene was removed, and the linkers with different lengths, (GSG)n (n = 1, 2) or (GGGGS)n (n = 1, 2), were introduced between the open reading frames of the YsADH and TkNOX genes via two rounds of PCR. The first round of PCR introduced the linkers (GSG)n (n = 1, 2) and (GGGGS)n (n = 1, 2) into the YsADH gene using four pairs of primers (Table 3). Simultaneously, the complementary linkers (GSG)n (n = 1, 2) and (GGGGS)n (n = 1, 2) were introduced into the TkNOX gene using four other pairs of primers (Table 3). Each PCR product was purified and served as a template in the second round of PCR. The PCR program included a 4 min period at 98 °C, 32 cycles at 98 °C (10 s), 58 °C (10 s) and 72 °C (30 s), and a final 5 min extension at 72 °C. The gel purified PCR products were ligated into a pACYCDuet-1 vector. Next, the PCR products of the YsADH and TkNOX genes were joined by overlapping extension PCR. The PCR program included a 4 min period at 98 °C, 32 cycles at 98 °C (10 s), 58 °C (10 s) and 72 °C (30 s), and a final 5 min extension at 72 °C. The gel purified PCR products were ligated into a pACYCDuet-1 vector. The four fusion genes were confirmed by sequencing. Finally, the four fusion genes were ligated to pACYCDuet-1 between NcoI and HindIII sites, yielding pACYCDuet-1-YsADH-(GGGGS)-TkNOX, pACYCDuet-1-YsADH-(GGGGS)2-TkNOX, pACYCDuet-1-YsADH-(GSG)-TkNOX and pACYCDuet-1-YsADH-(GSG)2-TkNOX. Using the construction of the plasmid pACYCDuet-1-YsADH-(GSG)-TkNOX as an example, the procedure was depicted in Additional file 1: Figure S5. Each expression construct pACYCDuet-1-YsADH-(GGGGS)-TkNOX, pACYCDuet-1-YsADH-(GGGGS)2-TkNOX, pACYCDuet-1-YsADH-(GSG)-TkNOX or pACYCDuet-1-YsADH-(GSG)2-TkNOX, was transformed into E. coli BL21(DE3) grown in LB medium containing 50 μg/ml chloramphenicol.
During the construction of YsADH-(linker)-TkNOX-(linker)-VsHGB fusion gene, the linker was chosen as GSG. Similar to the construction of YsADH-(linker)-TkNOX fusion genes, the fusion gene encoding YsADH-(GSG)-TkNOX-(GSG)-VsHGB or VsHGB-(GSG)-TkNOX-(GSG)-YsADH was obtained via two rounds of PCR and confirmed by sequencing. The fusion gene was ligated to pACYCDuet-1 between NcoI and HindIII sites and the resulting recombinant plasmid pACYCDuet-1-YsADH-(GSG)-TkNOX-(GSG)-VsHGB or pACYCDuet-1-VsHGB-(GSG)-TkNOX-(GSG)-YsADH. Using the construction of the plasmid pACYCDuet-1-YsADH-(GSG)-TkNOX-(GSG)-VsHGB as an example, the procedure was depicted in Additional file 1: Figure S6. Then, recombinant plasmid pACYCDuet-1-YsADH-(GSG)-TkNOX-(GSG)-VsHGB or pACYCDuet-1-VsHGB-(GSG)-TkNOX-(GSG)-YsADH was transformed into E. coli BL21(DE3) grown in LB medium containing 50 μg/ml chloramphenicol. Following the same procedure for the induction mentioned above, cells expressing the fusion enzyme YsADH-(linker)-TkNOX, YsADH-(GSG)-TkNOX-(GSG)-VsHGB or VsHGB-(GSG)-TkNOX-(GSG)-YsADH were induced, harvested and lyophilized.
Lyophilized cells were re-suspended in the 50 mM Tris-HCl buffer (pH 8.0) and disrupted through ultrasonication for 10 min. After that, the cell-debris pellet and cell-free extract were separated by 17,000 g centrifugation at 4 °C for 10 min. Then, the cell-debris pellet was re-suspended to the same volume of cell-free extract using the 50 mM Tris-HCl buffer (pH 8.0). Finally, the cell-debris pellet and cell-free extract samples were run by SDS-PAGE (12% acrylamide in the resolving gel) and stained with Coomassie Brilliant Blue R-250 .
TkNOX activities in cell-free extracts were determined according to the previously-reported procedure . YsADH activities in cell-free extracts were measured at 45 °C by monitoring the change of the absorbance at 340 nm. The enzyme assay for alcohol oxidation was carried out at 45 °C in triplicate in a reaction mixture (2.5 ml) composed of 20 mM crotyl alcohol and 1 mM NADP+ in 50 mM Tris-HCl (pH 8.0) buffer. The reaction was started by the addition of the enzyme. One unit of the activity is defined as formation or oxidation of 1 μmol NADPH per min. The protein concentrations of all samples were determined using the Bradford reagent with bovine serum albumin as the standard protein . In addition, the determination of H2O2 was conducted according to the previously-reported procedure .
The reaction mixture of α,β-unsaturated alcohol oxidation and its optimization
The setup of the reactor with hot plate/magnetic stirrer was shown in Additional file 1: Figure S7, in which the three-neck flask with magnetic stirring bar was used as a reaction vessel and the balloon was used to fill the atmosphere of reactor with oxygen. The standard reaction mixture (5 ml) contained 100 mM α,β-unsaturated alcohols, 0.3 g lyophilized cells, 0.4 mM NADP+, 0.2 mM FAD, 50 mM Tris-HCl buffer (pH 8.0). The reaction was carried out at 45 °C and 600 rpm for 2 h. The optimal temperature of alcohol oxidation was determined at a series of temperatures ranging from 40 to 65 °C. The optimal pH was determined over a range of pH 6.0 to 9.5 at 45 °C. The buffers used were PIPES (pH 6.0, 6.5 and 7.0), Tris-HCl (pH 7.5, 8.0, 8.5 and 9.0), and CAPS (pH 9.5). The optimal rotation was determined over a range of 400 to 900 rpm. FAD and NADP+ concentrations were explored within the range of 0 to 1 mM. After alcohol oxidation, the reaction mixture was extracted with 5 ml of ethyl acetate under strong vibration. The organic phase in samples was separated by 8000 g centrifugation at room temperature for 10 min and dehydrated by anhydrous sodium sulfate, and then 1 μl dehydrated sample was applied for GC analysis.
Determination of substrates, products and possible by-products by gas chromatograph
α,β-Unsaturated alcohols/aldehydes and possible by-products were determined by GC (Agilent 6890N) equipped with an FID detector and chiral capillary BGB-174 column (BGB Analytik, Böckten, Switzerland, 30 m × 250 µm × 0.25 µm). The flow rate and split ratio of N2 as the carrier gas were set as 1.38 ml/min and 1:100, respectively. Both injector and detector were kept at 250 °C. The injection volume was 1 µl.
For crotyl alcohol/crotonaldehyde, 3-methyl-2-buten-1-ol/3-methyl-2-butenal, trans-2-hexenol/trans-2-hexenal and cinnamyl alcohol/cinnamaldehyde, the column temperature program was listed as follows: initial temperature of 75 °C for 3 min, 10 °C/min ramp to 120 °C for 3 min, and 30 °C/min ramp to 180 °C for 3 min. For geraniol/geranal and nerol/neral, the column temperature program was listed as follows: initial temperature of 75 ° for 3 min, 4 °C/min ramp to 120 °C for 3 min, and 30 °C/min ramp to 180 °C for 3 min. The retention times of the above-mentioned substrates and products were summarized in Table 4.
For possible by-products isovaleraldehyde, isovaleric acid and 3,3-dimethylacrylic acid, the column temperature program was listed as follows: initial temperature of 60 °C for 5 min, 10 °C/min ramp to 120 °C for 3 min, and 30 °/min ramp to 180 °C for 3 min. The retention times for isovaleraldehyde, 3,3-dimethylacrylic acid and isovaleric acid were 6.987 min, 7.839 min and 9.612 min, respectively.
HPLC-based determination of retinol and retinal
Retinol and retinal were determined by HPLC (Waters 2010) equipped with an UV detector and C-18 column (Welch, 30 m × 250 µm × 0.25 µm). The HPLC conditions were listed as follows: Temperature, 40 °C; the wavelength of UV detector, 340 nm; mobile phase, methanol:acetonitrile = 95:5; flow rate, 1 ml/min. The retention times for retinol and retinal were 5.237 min and 5.618 min, respectively.
Availability of data and materials
The gene sequences in this study are available in the GenBank with Accession number of KF887947 for YsADH, BAD85488 for TkNOX and AAA27584 for VsHGB.
Alcohol dehydrogenase from Yokonella sp. WZY002
NADPH oxidase from Thermococcus kodakaraensis
Hemoglobin from Vitreoscilla stercoraria
Flavin adenine dinucleotide
Nicotinamide adenine dinucleotide phosphate
Sodium dodecyl sulfate polyacrylamide gel electrophoresis
Flame ionization detector
High performance liquid chromatography
Xing K, You K, Yin D, Yuan Z, Mao L. A simple and effificient approach for synthesis of pseudoionone from citral and acetone catalyzed by powder LiOH·H2O. Catal Commun. 2009;11:236–9.
Ventura CP. 3-Methyl-2-butenal. Synlett. 2010;17:2677–8.
de Almeida TP, van Schie MMCH, Ma A, Tieves F, Younes SHH, Fernández-Fueyo E, Arends IWCE, Riul A Jr, Hollmann F. Efficient aerobic oxidation of trans-2-hexen-1-ol using the aryl alcohol oxidase from Pleurotus eryngii. Adv Synth Catal. 2019;361:2668–72.
Hall E, Hauer B, Stuermer R, Kroutila W, Faber K. Asymmetric whole-cell bioreduction of an α, β-unsaturated aldehyde (citral): competing prim-alcohol dehydrogenase and C-C lyase activities. Tetrahedron Asymmetry. 2006;17:3058–62.
Kon Y, Usui Y, Sato K. Oxidation of allylic alcohols to a, b-unsaturated carbonyl compounds with aqueous hydrogen peroxide under organic solvent-free conditions. Chem Commun. 2007;42:4399–400.
Wang X, Liu R, Jin Y, Liang X. TEMPO/HCl/NaNO2 catalyst: a transition-metal-free approach to efficient aerobic oxidation of alcohols to aldehydes and ketones under mild conditions. Chem Eur J. 2008;14:2679–85.
Ying X, Wang Y, Xiong B, Wu T, Xie L, Yu M, Wang Z. Characterization of an allylic/benzyl alcohol dehydrogenase from Yokenella sp. strain WZY002, an organism potentially useful for the synthesis of α, β-unsaturated alcohols from allylic aldehydes and ketones. Appl Environ Microbiol. 2014;80:2399–409.
Mori S, Takubo M, Makida K, Yanase T, Aoyagi S, Maegawa T, Monguchi Y, Sajiki H. A simple and efficient oxidation of alcohols with ruthenium on carbon. Chem Commun. 2009; 5159–61.
Kroutil W, Mang H, Edegger K, Faber K. Biocatalytic oxidation of primary and secondary alcohols. Adv Synth Catal. 2004;346:125–42.
Dong J, Fernández-Fueyo E, Hollmann F, Paul CE, Pesic M, Schmit S, Wang Y, Younes S, Zhang W. Biocatalytic oxidation reactions: a chemist’s perspective. Angew Chem Int Ed. 2018;57:9238–61.
Liu J, Wu S, Li Z. Recent advances in enzymatic oxidation of alcohols. Curr Opin Chem Biol. 2018;43:77–86.
Kratzer R, Woodley JM, Nidetzky B. Rules for biocatalyst and reaction engineering to implement effective, NAD(P)H-dependent, whole cell bioreductions. Biotechnol Adv. 2015;33:1641–52.
Ying X, Ma K. Characterization of a zinc-containing alcohol dehydrogenase with stereoselectivity from the hyperthermophilic archaeon Thermococcus guaymasensis. J Bacteriol. 2011;193:3009–19.
Yu M, Huang M, Song Q, Shao J, Ying X. Characterization of a (2R,3R)-2,3-butanediol dehydrogenase from Rhodococcus erythropolis WZ010. Molecules. 2015;20:7156–73.
Zheng Y, Yin H, Yu D, Chen X, Tang X, Zhang X, Xue Y, Wang Y, Liu Q. Recent advances in biotechnological applications of alcohol dehydrogenases. Appl Microbiol Biotechnol. 2017;101:987–1001.
Ying X, Zhang J, Wang C, Huang M, Ji Y, Cheng F, Yu M, Wang Z, Ying M. Characterization of a carbonyl reductase from Rhodococcus erythropolis WZ010 and its variant Y54F for asymmetric synthesis of (S)-N-Boc-3-hydroxypiperidine. Molecules. 2018;23:3117.
Hummel W, Gröger H. Strategies for regeneration of nicotinamide coenzymes emphasizing self-sufficient closed-loop recycling systems. J Biotechnol. 2014;191:22–31.
Wu X, Kobori H, Orita I, Zhang C, Imanaka T, Xing X, Fukui T. Application of a novel thermostable NAD(P)H oxidase from hyperthermophilic archaeon for the regeneration of both NAD+ and NADP+. Biotechnol Bioeng. 2012;109:53–62.
Gao H, Li J, Sivakumar D, Kim T, Patel SKS, Kalia VC, Kim I, Zhang Y, Lee J. NADH oxidase from Lactobacillus reuteri: a versatile enzyme for oxidized cofactor regeneration. Int J Biol Micromol. 2019;123:629–36.
Li F, Zhou Q, Wei W, Gao J, Zhang Y. Switching the substrate specificity from NADH to NADPH by a single mutation of NADH oxidase from Lactobacillus rhamnosus. Int J Biol Macromol. 2019;135:328–36.
Liu S, Qi Q, Chao N, Hou J, Rao G, Xie J, Lu H, Jiang X. Overexpression of artificially fused bifunctional enzyme 4CL1-CCR: a method for production of secreted 4-hydroxycinnamaldehydes in Escherichia coli. Microb Cell Fact. 2015;14:118.
Chen K, Li K, Deng J, Zhang B, Lin J, Wei D. Carbonyl reductase identification and development of whole-cell biotransformation for highly efficient synthesis of (R)-[3,5-bis(trifluoromethyl)phenyl] ethanol. Microb Cell Fact. 2016;15:191.
Elleuche S. Bringing functions together with fusion enzymes—from nature’s inventions to biotechnological applications. Appl Microbiol Biotechnol. 2015;99:1545–56.
Zhang Y, Wang Y, Wang S, Fang B. Engineering bi-functional enzyme complex of formate dehydrogenase and leucine dehydrogenase by peptide linker mediated fusion for accelerating cofactor regeneration. Eng Life Sci. 2017;17:989–96.
Aalbers FS, Fraaije MW. Coupled reactions by coupled enzymes: alcohol to lactone cascade with alcohol dehydrogenase—cyclohexanone monooxygenase fusions. Appl Microbiol Biotechnol. 2017;101:7557–65.
Aalbers FS, Fraaije MW. Design of artificial alcohol oxidases: alcohol dehydrogenase-NADPH oxidase fusions for continuous oxidations. ChemBioChem. 2019;20:51–6.
Aalbers FS, Fraaije MW. Enzyme fusions in biocatalysis: coupling reactions by pairing enzymes. ChemBioChem. 2019;20:20–8.
Khosla C, Bailey JE. Characterization of the oxygen-dependent promoter of the Vitreoscilla hemoglobin gene in Escherichia coli. J Bacterol. 1989;171:5995–6004.
Nisar MA, Rashid N, Bashir Q, Gardner QA, Shafiq MH, Akhtar M. TK1299, a highly thermostable NAD(P)H oxidase from Thermococcus kodakaraensis exhibiting higher enzymatic activity with NADPH. J Biosci Bioeng. 2013;116:39–44.
Monti D, Ottolina G, Carrea G, Riva S. Redox reactions catalyzed by isolated enzymes. Chem Rev. 2011;111:4111–40.
Guo H, Yang Y, Xue F, Zhang H, Huang T, Liu W, Liu H, Zhang F, Yang M, Liu C, Lu H, Zhang Y, Ma L. Effect of flexible linker length on the activity of fusion protein 4-coumaroyl-CoA ligase::stilbene synthase. Mol BioSyst. 2017;13:598–606.
Ricca E, Brucher B, Schrittwieser JH. Multi-enzymatic cascade reactions: overview and perspectives. Adv Synth Catal. 2011;353:2239–62.
Nowak C, Beer B, Pick A, Roth T, Lommes P, Sieber V. A water-forming NADH oxidase from Lactobacillus pentosus suitable for the regeneration of synthetic biomimetic cofactors. Front Microbiol. 2015;6:957.
Ribeiro BD, Barreto DW, Coelho MAZ. Technological aspects of β-carotene production. Food Bioprocess Technol. 2011;11:693–701.
Millis JR, Saucy GG, Maurina-Brunker J, McMullin TW. Method of vitamin production. US patent 2002; US 6410755.
Wang C, Kima J, Choi E, Kim S. Microbial production of farnesol (FOH): current states and beyond. Proc Biochem. 2011;46:1221–9.
Dick M, Hartmann R, Weiergraber OH, Bisterfeld C, Classen T, Schwarten M, Neudecker P, Willboldbd D, Pietruszka J. Mechanism-based inhibition of an aldolase at high concentrations of its natural substrate acetaldehyde: structural insights and protective strategies. Chem Sci. 2016;7:4492–502.
Ying X, Wang C, Shao S, Wang Q, Zhou X, Bai Y, Chen L, Lu C, Zhao M, Wang Z. Efficient oxidation of methyl glycolate to methyl glyoxylate using a fusion enzyme of glycolate oxidase, catalase and hemoglobin. Catalysts. 2020;10:943.
Shapiro AL, Viñuela E, Maizel JV. Molecular weight estimation of polypeptide chains by electrophoresis in SDS-polyacrylamide gels. Biochem Biophys Res Commun. 1967;28:815–20.
Bradford MM. A rapid and sensitive method for the quantification of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem. 1976;72:248–54.
This work was supported by The Natural Science Foundation of Zhejiang Province, China (No. LY17B020012) and Xinmiao Talents Program of Zhejiang Province (No. 2020R403072).
The authors declare that they have no competing interests.
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The activities for YsADH and TkNOX in the cell-free extracts of whole-cell catalysts. Figure S1. SDS-PAGE analysis of cell-free extract and cell-debris pellet from the same whole catalyst comprising YsADH, TkNOX and/or VsHGB. Figure S2. SDS-PAGE analysis of cell-free extract and cell-debris pellet from the same whole catalyst comprising the fusion enzyme of YsADH and TkNOX. Figure S3. SDS-PAGE analysis of cell-free extract and cell-debris pellet from the same whole catalyst comprising the fusion enzyme of YsADH, TkNOX and VsHGB. Figure S4. The codon-optimized nucleotide sequences encoding YsADH (a), TkNOX (b) and VsHGB (c). Figure S5. The construction of the plasmid pACYCDuet-1-YsADH-(GSG)-TkNOX. Figure S6. The construction of the plasmid pACYCDuet-1-YsADH-(GSG)-TkNOX-(GSG)-VsHGB. Figure S7. The reactor with hot plate/magnetic stirrer (a) and its key components (b).
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Qiao, Y., Wang, C., Zeng, Y. et al. Efficient whole-cell oxidation of α,β-unsaturated alcohols to α,β-unsaturated aldehydes through the cascade biocatalysis of alcohol dehydrogenase, NADPH oxidase and hemoglobin. Microb Cell Fact 20, 17 (2021). https://doi.org/10.1186/s12934-021-01511-8
- α,β-Unsaturated aldehydes
- Alcohol dehydrogenase
- NADPH oxidase
- NADP+ regeneration
- Enzyme fusion