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A pyruvate carbon flux tugging strategy for increasing 2,3-butanediol production and reducing ethanol subgeneration in the yeast Saccharomyces cerevisiae
Biotechnology for Biofuelsvolume 11, Article number: 180 (2018)
The yeast Saccharomyces cerevisiae is a promising host cell for producing a wide range of chemicals. However, attempts to metabolically engineer Crabtree-positive S. cerevisiae invariably face a common issue: how to reduce dominant ethanol production. Here, we propose a yeast metabolic engineering strategy for decreasing ethanol subgeneration involving tugging the carbon flux at an important hub branching point (e.g., pyruvate). Tugging flux at a central glycolytic overflow metabolism point arising from high glycolytic activity may substantially increase higher alcohol production in S. cerevisiae. We validated this possibility by testing 2,3-butanediol (2,3-BDO) production, which is routed via pyruvate as the important hub compound.
By searching for high-activity acetolactate synthase (ALS) enzymes that catalyze the important first-step reaction in 2,3-BDO biosynthesis, and tuning several fermentation conditions, we demonstrated that a stronger pyruvate pulling effect (tugging of pyruvate carbon flux) is very effective for increasing 2,3-BDO production and reducing ethanol subgeneration by S. cerevisiae. To further confirm the validity of the pyruvate carbon flux tugging strategy, we constructed an evolved pyruvate decarboxylase (PDC)-deficient yeast (PDCΔ) strain that lacked three isozymes of PDC. In parallel with re-sequencing to identify genomic mutations, liquid chromatography–tandem mass spectrometry analysis of intermediate metabolites revealed significant accumulation of pyruvate and NADH in the evolved PDCΔ strain. Harnessing the high-activity ALS and additional downstream enzymes in the evolved PDCΔ strain resulted in a high yield of 2,3-BDO (a maximum of 0.41 g g−1 glucose consumed) and no ethanol subgeneration, thereby confirming the utility of our strategy. Using this engineered strain, we demonstrated a high 2,3-BDO titer (81.0 g L−1) in a fed-batch fermentation using a high concentration of glucose as the sole carbon source.
We demonstrated that the pyruvate carbon flux tugging strategy is very effective for increasing 2,3-BDO production and decreasing ethanol subgeneration in Crabtree-positive S. cerevisiae. High activity of the common first-step enzyme for the conversion of pyruvate, which links to both the TCA cycle and amino acid biosynthesis, is likely important for the production of various chemicals by S. cerevisiae.
The budding (brewer’s or baker’s) yeast Saccharomyces cerevisiae is a traditional microorganism used for various industrial applications. Historically, S. cerevisiae has mainly been used for alcohol (ethanol) fermentations (e.g., beer and wine) , but the use of this yeast as a microbial cell factory was recently proposed for producing a wide range of chemicals including higher alcohols (e.g., linear or branched alcohols and diols, such as 1-propanol , n-butanol , isobutanol  and 1,3-propanediol ). To date, the focus has mainly been on the production of 2,3-butanediol (2,3-BDO) [6,7,8,9] because it is relatively easy to engineer high-producing yeast strains due to their redox balanced NADH-dependent reductive reaction(s) (Fig. 1a–c) , the low toxicity of 2,3-BDO to microbes ), and the wide applicability of 2,3-BDO as a platform chemical (Fig. 1d).
2,3-BDO can be directly used as an anti-freeze agent or chemically converted to other chemicals (Fig. 1d) [10, 12]. For example, 1,3-butadiene (1,3-BD) can be produced by the two-step dehydration of 2,3-BDO [13, 14]. 1,3-BD is a feedstock for the generation of synthetic rubber , and for the synthesis of hexamethylene diamine and adipic acid . 2,3-BDO can also be converted to methyl ethyl ketone (MEK; butanone), 2-methylpropanal (2-MPA; isobutyraldehyde), and several butene derivatives by dehydration and/or hydrogenation (Fig. 1d). Thus, 2,3-BDO is a promising starting material for the synthesis of various compounds, including resin solvents, fuel additives, and butyl rubber (Fig. 1d) [13, 14, 17, 18].
The metabolic engineering of S. cerevisiae to produce various chemicals generally faces a common challenge: how to reduce dominant ethanol production . In the presence of a high concentration of glucose, S. cerevisiae produces ethanol dominantly, even under aerobic conditions, due to a process known as the “Crabtree effect” (Fig. 1a) [20, 21]. Increasing the concentration of glucose reduces the need for oxidative phosphorylation by the tricarboxylic acid (TCA) cycle and accelerates glycolysis as the major source of energy. Although the mechanism of this glycolytic overflow metabolism is not completely understood, it is assumed to involve the redox homeostasis of NADH between the glycolytic and fermentative (ethanol) pathways [20, 21], in which a net of two NADH molecules are generated from one glucose molecule via glycolysis and subsequently oxidized in the ethanol formation reaction ) (Fig. 1a). It has been experimentally demonstrated that increased NADH oxidation can reduce ethanol formation . Additionally, an in silico metabolic simulation suggested that the greater difficulty in metabolically engineering the eukaryote S. cerevisiae to produce higher alcohol concentrations compared to the prokaryote Escherichia coli is due to the structurally limited flexibility of the central metabolism and mitochondrial compartmentation of eukaryotes .
The NADH-dependent reductive reaction(s) may provide a strategy for using the 2,3-BDO biosynthesis pathway to displace the ethanol biosynthesis pathway (Fig. 1a) [10, 19]. In wild-type S. cerevisiae, 2-acetolactate is synthesized by the endogenous acetolactate synthase (ALS) Ilv2p, which localizes to the mitochondria and catalyzes the conversion of pyruvate (Fig. 1a) [12, 25]. Spontaneous decarboxylation can convert 2-acetolactate into diacetyl in the presence of oxygen. Next, diacetyl can be converted in the yeast cytosol into acetoin and 2,3-BDO via the NADH-dependent two-step reductive reactions of butanediol dehydrogenase (BDH; EC 22.214.171.124), an enzyme that also has diacetyl reductase activity and is encoded by the BDH1 (or BDH2) gene in S. cerevisiae (Fig. 1a) . In contrast, many bacteria synthesize 2-acetolactate in the cytosol (Fig. 1b) and then convert it into acetoin via two routes: (1) a two-step conversion by spontaneous decarboxylation and an NADH-dependent diacetyl reductase reaction (Fig. 1b), or (2) an enzymatic one-step conversion by acetolactate decarboxylase (ALDC) (Fig. 1c) . Similar to S. cerevisiae, bacteria also further convert acetoin into 2,3-BDO by an NADH-dependent BDH reductive reaction . Although redox balance is not completely maintained in the bacterial ALDC reaction, moderate production of 2,3-BDO is possible.
To achieve increased production of higher alcohols and reduced subgeneration of ethanol in Crabtree-positive S. cerevisiae, in this study we investigated the utility of tugging high glycolytic carbon flux into 2,3-BDO biosynthesis by introducing a stronger pulling effect at the hub branching point (pyruvate) (Fig. 1b). For this purpose, we searched gene databases for a high-activity ALS enzyme and confirmed the effectiveness of the identified enzyme for increasing 2,3-BDO production and reducing ethanol subgeneration. We demonstrated the validity of our strategy by constructing a pyruvate decarboxylase (PDC)-deficient yeast (PDCΔ) strain and conducted experimental evolution to improve its growth rate (Fig. 1c). In parallel with genome re-sequencing for identifying mutations, we conducted liquid chromatography–tandem mass spectrometry (LC–MS/MS) analysis of the intermediate metabolites. This analysis revealed significant accumulation of pyruvate and NADH in the evolved PDCΔ strain. The combination of the high-activity ALS and the manipulation of additional downstream enzymes for 2,3-BDO biosynthesis into this evolved PDCΔ strain provided a high yield of 2,3-BDO (a maximum of 0.41 g g−1 glucose consumed, the highest value reported to date for S. cerevisiae [12, 26]). Using this engineered strain, we tuned the fermentation conditions and achieved a quite high 2,3-BDO titer (81.0 g L−1) in fed-batch fermentations using a high concentration of glucose as the sole carbon source.
Yeast strains and media
Full details of the culture media are described in Additional file 3: Method S1. Briefly, yeast–peptone–dextrose–adenine (YPDA), minimal synthetic dextrose (SD), and synthetic complete (SC) media containing 20 g L−1 glucose were used. For fermentation tests, SD medium contained a high concentration of glucose (25, 50 or 100 g L−1) as the sole carbon source. Amino acids and nucleotides were supplemented as necessary because SD selection medium lacks these auxotrophic components.
Yeast strain construction
Full details of the construction of the gene deletion mutants are described in Additional file 3: Method S2 and are shown in Additional file 1: Fig. S1. All yeast strains used in this study were generated from the YPH499 parental strain  and are listed in Table 1. All primers used for the construction of the yeast gene deletion mutants are listed in Additional file 2: Table S1. Using YPH499 as the parental strain, a quadruple deletion mutant (MTH1-ΔT pdc1Δ pdc5Δ pdc6Δ) YSM021 strain (PDCΔ strain) (Table 1) was constructed using the seamless marker recycling method (URA-blaster method) .
Plasmid construction and yeast transformation
Full details regarding plasmid construction and yeast transformation are described in Additional file 3: Method S3. All plasmids used in this study are listed in Table 2. All primers used for plasmid construction are listed in Additional file 2: Table S1. The transformation of plasmid DNA was carried out using the lithium acetate method . All transformants generated in this study are listed in Table 3.
Full details of the laboratory evolution experiments are described in Additional file 3: Method S4. For laboratory evolution of the PDCΔ (YSM021) strain (Table 1), a passage culture in SD medium was carried out with five independent culture series. Cells of culture series 1 at days 44 and 122 (Evo44 and Evo122 strains) (Table 1) were stored as glycerol stocks. An isolate of Evo122 (Evo122-2) was designated the YSM046 strain (evolved PDCΔ strain) (Table 1).
Full details of the genome re-sequencing experiments are described in Additional file 3: Method S5. The whole genomes of YPH499, YSM021, and six evolved strains were sequenced by pair-end sequencing (250 bp) using an Illumina HiSeq2000 next-generation sequencer and a MiSeq reagent 500 cycle kit v2 (Illumina, San Diego, CA, USA), then analyzed with Bowtie2 , SAMtools , and Integrative Genomics Viewer (IGV)  software.
Relative activity measurements of acetolactate synthase (ALS) enzymes
Full details of the ALS enzyme assays are described in Additional file 3: Method S6). Yeast cells were grown in SD selection medium and then the collected cells were disrupted with glass beads using a Shake Master Neo (Bio Medical Science, Tokyo, Japan) to obtain cell crude extracts. The ALS activity assay basically followed previously described procedures [33, 34]. Briefly, a pre-mixture containing thiamine pyrophosphate, FAD, MgCl2 and crude yeast cell extract was pre-incubated, and then the reaction was started by adding pyruvate. The reaction was stopped by adding sulfonic acid and the reaction mixture was incubated to convert 2-acetolactate to acetoin. Acetoin was then further oxidized to diacetyl with creatine and α-naphthol. The relative ALS activity based on the colorimetric assay of acetoin (or diacetyl) was determined by measuring the absorbance (at 525 nm) of the developed red color using an EnVision multilabel plate reader (Perkin Elmer, Waltham, MA, USA).
Full details of the culture conditions are described in Additional file 3: Method S7. Yeast cells were seeded at a low initial optical density (OD) and grown or used for fermentation in SD or SD selection media containing 20 g L−1 glucose at 30 °C. The fermentation conditions of the YHI030 strain (Table 2) were tuned by inoculating the pre-cultured cells into 50 mL of fresh SD selection medium (containing either 25, 50 or 100 g L−1 glucose) to give an initial cell density of 15 g L−1 (wet cell weight). Buffer medium was pH-adjusted by adding 2-(N-morpholino)ethanesulfonic acid (MES) to the SD selection medium. Additional glucose was added to the fermented culture for fed-batch fermentations.
Analysis of extracellular metabolites
Full details of the analysis of extracellular metabolites are described in Additional file 3: Method S8. The concentrations of 2,3-BDO, glucose, ethanol, glycerol, acetoin, pyruvate, acetate, lactate and succinate in the culture medium were determined using a high-performance liquid chromatography (HPLC) system (with UV/Vis and refractive index detectors) (Shimadzu, Kyoto, Japan) equipped with an Aminex HPX-87H column (300 × 7.8 mm) (Bio-Rad, Hercules, CA, USA).
LC–MS/MS analysis of intermediate metabolites
Selection of acetolactate synthase (ALS) for 2,3-BDO biosynthesis
ALS is the first-step enzyme in valine biosynthesis, catalyzes the conversion of pyruvate to 2-acetolactate, and is important for 2,3-BDO biosynthesis (Fig. 1a, b) [4, 36]. To tug the carbon flux from pyruvate and enhance 2,3-BDO biosynthesis in S. cerevisiae, we isolated the genes encoding ALS enzymes from various species. Sixteen ALS genes from 11 species other than S. cerevisiae (12 genes were from eight prokaryotes and 4 genes were from three eukaryotes) were cloned into the pGK425 yeast expression vector  (Table 2) and expressed under the PGK1 promoter in YPH499 (wild-type) yeast strain (Table 3). The relative ALS activities of crude cell extracts were measured after 48 h of cultivation (Fig. 2). ILV2 (encoding the endogenous S. cerevisiae ALS ) and ILV2c (a truncated version of the ILV2 gene lacking the mitochondrial signal sequence to localize Ilv2 in cytosol ) genes (Fig. 1a, b) were used as positive controls to assess the capabilities of the ALS enzymes. Most of the constructed strains showed higher ALS activities than the control strain (harboring the mock control vector) that inherently contains the ILV2 gene in the genome (Fig. 2). Eight strains exhibited higher ALS activities than the strain expressing the truncated (cytosolic) ILV2c gene, and five strains displayed higher ALS activities than the strain overexpressing the intact (mitochondrial) ILV2 gene. The relative measured ALS activities were used to identify the top three genes as alsLp (from Lactobacillus plantarum; 27.8-fold), ilvBEc (from Escherichia coli; 5.5-fold) and alsTf (from Thermobifida fusca; 2.8-fold). Notably, the alsLp gene encoded an enzyme with much higher ALS activity than any other ALS tested (Fig. 2).
The top three ALS genes were introduced into yeast cells and 2,3-BDO fermentations were performed in test tubes (Fig. 3a). Strains harboring the mock vector and the ILV2c expression plasmid were, respectively, used as negative and positive controls. The alsLp, ilvBEc and alsTf genes were codon-optimized (alsLpOp, ilvBEcOp and alsTfOp), subcloned into the same pGK425 expression vector (Table 2), and introduced into YPH499 (Table 3). The obtained strains were cultured in test tubes with 3 mL of SD medium (containing 20 g L−1 glucose) under semi-aerobic conditions (Fig. 3a). The expression of ILV2c in YPH499 resulted in a four-time higher 2,3-BDO titer (141 mg L−1) compared to the negative control strain (35 mg L−1), and expression of the top three ALS genes further increased the titer of 2,3-BDO. The increased levels of 2,3-BDO correlated with the strength of the relative ALS activity (Fig. 2). YPH499 strain expressing the alsLpOp gene yielded 403 mg L−1 2,3-BDO, while those expressing the ilvBEcOp or alsTfOp genes produced 223 and 188 mg L−1 2,3-BDO (Fig. 3a), respectively. The strain expressing alsLpOp resulted in a slight decrease in ethanol concentration (7.0 g L−1) compared to the mock control strain (8.1 g L−1) and the strain expressing ILV2c (7.7 g L−1) (p < 0.05; Fig. 3a).
Demonstration of the tugging of pyruvate flux by simple tuning using a high-activity ALS-expressing wild-type strain
We increased the titer of 2,3-BDO and reduced ethanol subgeneration by further tuning the wild-type yeast strain expressing a high-activity ALS (alsLpOp) by introducing the expression of additional genes (ALDC genes and BDH1) and altering the aeration conditions (Additional file 1: Fig. S2, Fig. 3b, c). Co-expression of the alsLpOp and ALDC (codon-optimized) genes from several bacteria using the pATP422 multiple gene expression vector  (Table 2) in YPH499 (Table 3; YIDB030–033) did not result in an increase in 2,3-BDO compared to the strain expressing only the alsLpOp gene (Additional file 1: Fig. S2). This decrease in productivity might be attributed to the reduced consumption of NADH in 2,3-BDO biosynthesis via the ALDC reaction (Fig. 1c). Briefly, the ALDC pathway does not use NADH to convert 2-acetolactate to acetoin (Fig. 1c), while the alternative diacetyl pathway uses NADH through the reaction of diacetyl reductase (encoded by BDH1 in S. cerevisiae) (Fig. 1b). Consequently, the overexpression of ALDC might decrease carbon flux toward 2,3-BDO to consume excess NADH during ethanol biosynthesis. Indeed, the ALDC-expressing strains produced higher amounts of ethanol than the non-expressing strain (data not shown).
Culture conditions (aeration) were investigated by changing the agitation speed (150–300 rpm) and the cover cap on the test tubes (aluminum cap to a vent-type cap, SILICOSEN®) using the YPH499 strain expressing the ALS (alsLpOp) gene (Fig. 3b). Under the same conditions as used for the previous cultures (aluminum cap, 150 rpm), the strain produced 494 mg L−1 2,3-BDO and 8.8 g L−1 ethanol. The titers of YPH499 expressing the ALS (alsLpOp) gene slightly differed from those shown in Fig. 3a, possibly due to differences between the vector backbones (pGK425 and pATP422 in Fig. 3a, b, respectively). As aeration increased (aluminum cap and vent-type cap, 300 rpm), significant decreases in ethanol production were observed (6.2 and 3.7 g L−1) (Fig. 3b). A moderate increase in aeration (aluminum cap, 300 rpm) resulted in a higher 2,3-BDO production titer (711 mg L−1), whereas a large increase in aeration (vent-type cap, 300 rpm) reduced the 2,3-BDO titer (256 mg L−1) (Fig. 3b). It is possible that excessive aeration (vent-type cap, 300 rpm) may have resulted in the redirection of pyruvate flux towards the TCA cycle, faster respiration, and/or the evaporation of ethanol. Regardless, YPH499 expressing the ALS (alsLpOp) gene under high aeration conditions produced ethanol titers consistent with previous reports [20, 21]. In contrast, conditions of reduced aeration (aluminum cap, 300 rpm) could have reduced the spontaneous decarboxylation required for converting 2-acetolactate to diacetyl because this reaction requires moderate concentrations of oxygen .
BDH1, which encodes endogenous yeast BDH, was overexpressed along with alsLpOp using the pATP422 multiple gene expression vector (Table 2) in YPH499 (Table 3; YIDB034), resulting in the 2,3-BDO titer increasing up to 874 mg L−1 (p < 0.05; Fig. 3c). The titer of ethanol was reduced to 5.1 g L−1 (p < 0.05; Fig. 3c) because the carbon flux to 2,3-BDO biosynthesis was further enhanced by the additional expression of Bdh1 enzyme (Fig. 1b). These results demonstrated the validity of the pyruvate carbon flux strategy for 2,3-BDO production in the wild-type strain using high-activity ALS (the alsLpOp gene). However, this engineered strain (expressing the alsLpOp and BDH1 genes) still exhibited a high titer of ethanol. Consequently, the disruption of ethanol biosynthesis is a strategy for tugging pyruvate carbon flux and further improving 2,3-BDO production.
Construction of a pyruvate decarboxylase-deficient (PDCΔ) strain (YSM021 strain)
Full details of the results for constructing the PDCΔ (YSM021) strain are described in Additional file 3: Result S1. Briefly, we disrupted ethanol biosynthesis by following the strategy used to construct the previously reported pyruvate decarboxylase-deficient Pdc− strain (deletion of the coding DNA sequence (CDS) regions of the PDC1, PDC5 and PDC6 genes, and introduction of the MTH1-ΔT allele) . We constructed the pyruvate decarboxylase-deficient PDCΔ strain YSM021 (Table 1) from YPH499, and confirmed quadruple gene deletion (MTH1-ΔT pdc1Δ pdc5Δ pdc6Δ) by genome re-sequencing (Fig. 4a–d). The genome sequence of YSM021 strain further revealed the occurrence of a nonsynonymous substitution (L165F) in the MTH1-ΔT gene due to a single nucleotide polymorphism (SNP) located at position 468 (from A to C) (Fig. 4d, Table 1). Although the glucose consumption of YSM021 was much slower than that of YPH499, no ethanol, glycerol, or acetate production was detected in YSM021 cultures after 120 h of cultivation (Additional file 1: Fig. S3) but pyruvate accumulated with time (Additional file 1: Fig. S3).
Laboratory evolution of the PDCΔ strain and genome re-sequencing
Full details of the laboratory evolution of the PDCΔ (YSM021) strain and genome re-sequencing are described in Additional file 3: Result S2. Briefly, laboratory evolution of the PDCΔ (YSM021) strain using a series of five independent cultures allowed for faster growth of culture series 1 (Additional file 1: Fig. S4). Three colonies isolated from the cells collected at days 44 and 122 (Evo44 and Evo122) (Table 1) showed improved cell growth phenotypes (Fig. 5).
Genome re-sequencing revealed several nonsynonymous mutations, including an A to T mutation at position 1547 (D516V) in the YAK1 gene (YJL141C) and a G to A mutation at position 605 (G202D) in the MCT1 gene (YOR221C) (Table 4). MCT1 is predicted to encode a malonyl-CoA:ACP transferase responsible for lipid biosynthesis . YAK1 encodes a serine–threonine protein kinase that inhibits growth in response to glucose availability in a glucose-sensing system [42, 43], suggesting that the mutation in YAK1 is likely responsible for the observed improved cell growth rate. Further genetic characterization of these mutations (including L165F in the MTH1-ΔT gene) is in progress and will be reported elsewhere in the future.
An isolate of Evo122 (Evo122-2) was designated as YSM046 (Table 1) and used for 2,3-BDO production. A comparison of culture profiles indicated that the cell growth rate of YSM046 strain was significantly improved compared to YSM021, and ethanol and glycerol were not produced (Additional file 1: Fig. S3).
Metabolic state of the evolved PDCΔ strain (YSM046 strain)
The state of central carbon metabolism in the evolved strain was investigated by metabolic profiling analysis. The wild-type strain (YPH499) and the evolved strain (YSM046, PDCΔ + evolved) (Table 1) were cultivated in shake flasks with 100 mL SD medium under aerobic conditions (Fig. 6). Glucose was slowly consumed by the YSM046 strain and no ethanol and little glycerol were produced (Fig. 6), consistent with the small-scale cultivation data (Additional file 1: Fig. S3). The specific growth rates of YPH499 and the evolved strain YSM046 were 0.30 ± 0.003 and 0.091 ± 0.002 h−1, respectively. Intracellular metabolites were extracted from cells collected at mid-log phase (OD660 = 1.0; see “Methods” for the detailed procedure) and metabolite concentrations were determined by ion-pairing LC–MS/MS analysis (Fig. 7).
Comparison of the pool sizes of glycolytic intermediates and cofactors indicated that two substrates for the PDC (pyruvate decarboxylase) and ADH (alcohol dehydrogenase) reactions, pyruvate and NADH, significantly accumulated (3.9- and 3.2-fold, respectively) in the evolved PDCΔ strain YSM046 cells (Fig. 7). The reduced levels of energy charge (decreased ATP and increased ADP) and fructose 1,6-bisphosphate (FBP: only 15.3% that of YPH499) in YSM046 cells suggested that the low ATP level should have affected the activity of phosphofructokinase (fructose 6-phosphate (F6P) + ATP → FBP + ADP), resulting in slower glycolysis in the YSM046 strain. However, the level of pyruvate accumulation was suitable for demonstrating our strategy and thus we further exploited the YSM046 strain to validate the utility of tugging the pyruvate flux for 2,3-BDO production.
Construction of 2,3-BDO-producing evolved PDCΔ strains harboring high-activity ALS and downstream aldcLlOp and BDH1 genes (YHI030 strain)
Saccharomyces cerevisiae strains producing 2,3-BDO were constructed by introducing the high-activity ALS (alsLpOp) gene and/or the downstream (ALDC and BDH; aldcLlOp and BDH1) genes for 2,3-BDO biosynthesis into the YSM046-evolved PDCΔ strain (YHI010, YHI011 and YHI030; Table 3) and the YPH499 wild-type strain (YHI027; Table 3). The strains were cultured in 5 mL of SD selection medium under semi-aerobic conditions. The concentrations of 2,3-BDO and other compounds 96 h after the start of fermentation are shown in Fig. 8.
Both glucose consumption and 2,3-BDO titer were increased by sequential introduction of the alsLpOp, aldcLlOp and BDH1 genes into the YSM046 strains (Fig. 8). The 2,3-BDO titer of YHI030 strain (YSM046 strain expressing alsLpOp, aldcLlOp and BDH1) was 6.6 ± 2.2 g L−1 (0.41 g g−1 glucose consumed), comparable to the highest value reported for S. cerevisiae [12, 26]). We observed no over-production of 2,3-BDO by YHI027 strain expressing the same (alsLpOp, aldcLlOp and BDH1) genes present in wild-type YPH499 (0.37 ± 0.05 g L−1; 0.02 g g−1 glucose consumed). No ethanol was detected in the culture media of the YSM046-derived strains (YHI030, YHI011 and YHI010) whereas YHI027 strain produced 3.7 ± 0.3 g L−1 ethanol as the major product. YHI030 showed slightly higher (1.7-fold) glycerol production than YHI027 (Fig. 8), probably due to an excess of NADH resulting from the loss of ethanol biosynthesis. The higher growth rate of the evolved PDCΔ strain (YSM046) compared to the non-evolved PDCΔ strain (YSM021) was confirmed, even when YSM046 expressed the alsLpOp, aldcLlOp and BDH1 genes (Table 3, Additional file 1: Fig. S5). These results indicate that the YSM046-evolved PDCΔ strain is useful as a host strain for tugging pyruvate carbon flux and increasing 2,3-BDO production, although its growth rate requires improvement prior to industrial application.
2,3-BDO production by fermentation using YHI030 strain
2,3-BDO was further produced by fermentation using the YHI030 strain. Small fermentation bottles containing SD selection medium and several high concentrations of glucose (25, 50 and 100 g L−1) as the sole carbon source were used to generate oxygen-limited (anaerobic) conditions.
The cells almost completely consumed 25 and 50 g L−1 glucose after 24 and 48 h of fermentation, respectively (Fig. 9a, b). After 48 and 72 h of fermentation, the 2,3-BDO titer of YHI030 strain was 9.1 ± 0.4 g L−1 (0.37 g g−1 glucose consumed) and 17.4 ± 0.3 g L−1 (0.35 g g−1 glucose consumed), respectively, from 25 and 50 g L−1 glucose, and the glycerol titer was, respectively, 7.4 ± 0.2 g L−1 (0.30 g g−1 glucose consumed) and 15.3 ± 0.6 g L−1 (0.31 g g−1 glucose consumed). Although the cells produced 22.1 ± 1.1 g L−1 2,3-BDO (0.38 g g−1 glucose consumed) and 19.7 ± 1.6 g L−1 glycerol (0.34 g g−1 glucose consumed) from 100 g L−1 glucose after 96 h of fermentation, the glucose consumption rate decreased after 48 h and the 100 g L−1 of glucose was not completely consumed (Fig. 9c). For all concentrations of glucose, the yields of 2,3-BDO and glycerol were, respectively, 0.35–0.38 and 0.30–0.34 g g−1 glucose consumed, whereas very low levels of the other metabolites measured (ethanol, acetate, lactate, succinate and pyruvate) were detected in the fermentation media. The relatively high levels of glycerol generation were probably caused by the excess of NADH arising from deficient ethanol biosynthesis (similar to the results shown in Fig. 8).
Investigation of fermentation conditions for 2,3-BDO production by YHI030 strain
Since not all the 100 g L−1 glucose was consumed during fermentation (Fig. 9c), we investigated the effects of adding glucose in a step-by-step manner (Additional file 1: Fig. S6). During anaerobic fermentation, 50 or 25 g L−1 glucose was added to the culture in incremental steps (Additional file 1: Fig. S6A and B). In both cases, the cells showed decreased glucose consumption after the addition of a total of 50 g L−1 glucose. The 2,3-BDO titer remained static at around 20 g L−1.
Subsequently, we tested the effect of aerobic fermentation in SD selection medium (50 and 100 g L−1 glucose) using Erlenmeyer flasks and different agitation speeds (100 and 200 rpm) (Additional file 1: Fig. S7). At 100-rpm agitation, YHI030 strain produced approximately 20 g L−1 2,3-BDO in medium containing initially either 50 or 100 g L−1 glucose (Additional file 1: Fig. S7A and B); in medium containing initially 100 g L−1 glucose, the cells consumed approximately 40 g L−1 glucose (Additional file 1: Fig. S7B). The production of glycerol was significantly reduced when fermentation was conducted in medium containing initially either 50 or 100 g L−1 glucose and agitated at 100 rpm (4.7 and 7.2 g L−1 glycerol, respectively) (Additional file 1: Fig. S7A and B).
The fermentation of either 50 or 100 g L−1 glucose under more aerobic conditions (200 rpm) resulted in lower 2,3-BDO production (~ 14 g L−1) and decreased glucose consumption (~ 30 g L−1) (Additional file 1: Fig. S7C and D), indicating that conditions approximating an oxygen-limited aerobic state are suitable for 2,3-BDO production by YHI030 strain. Furthermore, all cultures showed increased cell densities (OD = 20–25) and a significant decrease in pH (2–3) after 24 h of fermentation (Additional file 1: Fig. S7C and D). Fermentation at 300 rpm in medium containing 50 or 100 g L−1 glucose resulted in 2,3-BDO production profiles similar to those at obtained at 200 rpm (data not shown).
We investigated the effect of severely decreased pH on the production of 2,3-BDO by adding 200 mM MES buffer to the fermentation medium and adjusting the pH to 6.0, then conducting fermentation using milder agitation speeds (50, 100 and 150 rpm). We found that YHI030 strain rapidly and completely consumed 50 g L−1 glucose at each agitation speed tested (Additional file 1: Fig. S8). The cells produced approximately 14 g L−1 2,3-BDO and 5 g L−1 glycerol during fermentation conducted at 100 and 150 rpm (Additional file 1: Fig. S8B and C), whereas at 50 rpm, the cells produced 17.6 g L−1 2,3-BDO but no significant reduction in glycerol was observed (Additional file 1: Fig. S8A). The cell density was increased (OD = 25–28) and the pH was moderately decreased (pH = 3.5–4.5) during fermentation at 100 and 150 rpm but remained essentially unchanged (OD = 18–19, pH = 5.2–5.4) at 50 rpm.
YHI030 strain produced 34–39 g L−1 2,3-BDO after 72–96 h of fermentation in pH-adjusted buffered medium containing 100 g L−1 glucose (Additional file 1: Fig. S9). At 50 rpm, the glucose was almost entirely consumed at 72 h (Additional file 1: Fig. S9A), whereas more than 10–15 g L−1 glucose remained after 96 h of fermentation at 100 and 150 rpm (Additional file 1: Fig. S9B and C). Similar to fermentation in the presence of 50 g L−1 glucose, the cell density and pH of cultures agitated at 50 rpm in the presence of 100 g L−1 glucose remained essentially constant whereas the cell densities of cultures agitated at 100 and 150 rpm were increased and the pH values of the media were decreased.
Fed-batch fermentation by YHI030 strain for the production of 2,3-BDO by adding a high concentration of glucose
Finally, we again tested the step-by-step addition of glucose as the sole carbon source to medium buffered with 500 mM MES (pH 6.0) (Fig. 10). During aerobic fermentation with 50-rpm agitation (mild aerobic conditions), 300 g L−1 glucose was added to the fermentation culture in three equal doses (100 g L−1 each). YHI030 strain consumed the initial 100 g L−1 glucose and produced 36.2 ± 1.7 g L−1 2,3-BDO at 72 h (Fig. 10). The cells consumed an additional 100 g L−1 glucose (total 200 g L−1) and produced 61.7 ± 1.3 g L−1 2,3-BDO at 120 h after the first glucose addition (total 192 h). Finally, the cells almost completely consumed a further additional 100 g L−1 glucose (total 300 g L−1) and the 2,3-BDO titer reached 81.0 ± 1.3 g L−1 at 312 h after the second glucose addition (total 504 h). The highest yield of 2,3-BDO in each (1st, 2nd and 3rd) fermentation step was 0.38 (at 72 h), 0.35 (at 96 h; total 168 h), and 0.27 (at 312 h; total 504 h) g g−1 glucose consumed. The glycerol titers were 32.3 ± 0.7 g L−1 (at 72 h), 55.3 ± 0.7 g L−1 (at 120 h; total 192 h) and 71.8 ± 0.7 g L−1 (at 312 h; total 504 h). The cells produced small amounts of succinate (1.3, 3.3 and 4.0 g L−1) and pyruvate (0.6, 1.0 and 1.0 g L−1) (at 72 h, at 120 h; total 192 h, and at 312 h; total 504 h), but ethanol, acetate or lactate were not detected. The cell density remained essentially unchanged during the fermentation and pH gradually decreased to between pH 5 and 6 (Fig. 10).
The aim of this study was to develop a yeast metabolic engineering strategy for increasing higher alcohol production and concomitantly reducing ethanol subgeneration. To this end, we proposed a methodological approach for tugging the carbon flux in central metabolism at an important hub branching point (e.g., pyruvate and acetyl-CoA). We verified the validity of this strategy by testing 2,3-BDO production, which requires pyruvate as the hub branching point.
First, we ensured that pyruvate flux would be tugged towards 2,3-BDO biosynthesis by searching various ALS (acetolactate synthase) candidates to serve as the common first-step enzyme for the conversion of pyruvate to 2,3-BDO. We identified a high-activity ALS gene from L. plantarum (alsLp) by analyzing crude yeast cell extracts using an enzyme activity assay (Fig. 2). The high-activity alsLp gene was codon-optimized (alsLpOp) and its feasibility for 2,3-BDO production was tested. Expression of the alsLpOp gene in YPH499 wild-type strain resulted in a higher titer of 2,3-BDO production compared to the expression of other ALS genes, including endogenous yeast ILV2 (mitochondria)  and ILV2c (cytosol)  (Fig. 3a). Simple tuning of aeration and BDH expression resulted in a significant increase and decrease in 2,3-BDO production and ethanol subgeneration, respectively (Fig. 3b, c). Thus, we validated the strategy of pyruvate carbon flux tugging using high-activity ALS for increasing higher alcohol production (2,3-BDO) in the wild-type strain.
However, substantial ethanol production was still observed and thus we generated the evolved PDCΔ YSM046 strain by quadruple deletions (MTH1-ΔT allele and PDC1, 5, 6Δ) and laboratory evolution. LC–MS/MS analysis was used to compare the pool sizes of glycolytic intermediates and cofactors (Fig. 7) and showed that YSM046 is a promising strain for the production of 2,3-BDO and other compounds (e.g., lactate  and butanol ) because YSM046 significantly accumulated pyruvate and NADH, the precursor and cofactor required for the biosynthesis of various metabolites [23, 45]. However, the specific growth rate of evolved PDCΔ strain YSM046 was 0.091 ± 0.002 h−1 (from 20 g L−1 glucose under aerobic conditions), which is significantly slower than that of previously reported Pdc− strains with similar MTH1-ΔT alleles (cultured in aerobic, pH-controlled bioreactors in medium containing 7.5 g L−1 glucose: 0.10 h−1 without evolution and 0.20 h−1 with evolution) [40, 46]. The same Pdc− strains showed higher specific growth rates (0.24 and 0.23 h−1, respectively) following the addition of a small amount of ethanol (0.3%, v/v), whereas the original PDC-deficient yeast strain (without the MTH1-ΔT allele) could not grow in the presence of a high glucose concentration as the sole carbon source and required C2 compounds (ethanol or acetate) for growth under low glucose concentrations. The necessity for C2 compounds may be due to the inability to synthesize cytosolic acetyl-CoA from pyruvate [40, 46,47,48]. Thus, the addition of C2 compounds might improve both cell growth and 2,3-BDO production by PDCΔ strains at high glucose concentrations.
YSM046 (evolved PDCΔ) strain accumulated significant amounts of pyruvate (and NADH) and dramatically increased 2,3-BDO production by expressing alsLpOp, aldcLlOp and BDH1 (Fig. 8). In contrast to YPH499 wild-type strain (Additional file 1: Fig. S2), the additional expression of ALDC (acetolactate decarboxylase; aldcLlOp) by YSM046 strain substantially improved 2,3-BDO productivity (Fig. 8). This evolved PDCΔ strain (YSM046) did not produce ethanol (Figs. 6 and 8) and thus the accumulated pyruvate (Fig. 7) could be used to consume glycolysis-derived NADH (or to regenerate NAD+). This excess pyruvate could be removed by converting 2-acetolactate to acetoin through spontaneous decarboxylation and subsequent reduction (via diacetyl) (Fig. 1b). This diacetyl pathway (Fig. 1b) is more balanced in terms of redox equilibrium than the ALDC pathway (Fig. 1c); however, the diacetyl pathway might have a limited capacity in 2-acetolactate conversion reaction. Consequently, expression of the ALDC enzyme likely aided the consumption of excess pyruvate during 2,3-BDO biosynthesis, despite the relatively poor redox balance (Fig. 1c).
The 2,3-BDO titer and yield of YHI030 strain (YSM046-evolved PDCΔ strain expressing the alsLpOp, aldcLlOp and BDH1 genes) were 6.6 ± 2.2 g L−1 and 0.41 g g−1 consumed glucose, respectively. The 2,3-BDO titer generated by YHI030 strain was increased 17.8-fold compared to YHI027 strain (and 20.5-fold based on consumed glucose) by introducing the PDCΔ genotype and through evolutionary engineering. These data clearly demonstrate the utility of our strategy using pyruvate flux tugging for 2,3-BDO production. In addition, this yield is comparable to the highest yield reported for an engineered S. cerevisiae strain [12, 26]. In brief, the ADH- and NAD-dependent glycerol-3-phosphate dehydrogenase (GPD) enzymes were deleted from this previously reported strain (adh1–5Δ and gpd1–2Δ) and the noxE (NADH oxidase from Lactococcus lactis), alsS (ALS from Bacillus subtilis), alsD (ALDC from B. subtilis) and BDH1 (S. cerevisiae) genes were inserted. This strain achieved a high yield of 2,3-BDO (72.9 g/L) at 0.41 g g−1 glucose consumed (fed-batch) by eliminating byproduct formation (GPD deletion) and redox rebalancing (noxE expression).
Finally, 2,3-BDO fermentation using a high density of YHI030 strain cells (15 g L−1; wet cell weight) and a high concentration of glucose as the sole carbon source was tested under various fermentation conditions (Figs. 9, 10, and Additional file 1: Figs. S6–S9). Under mild aerobic conditions (at an agitation of 50 rpm) in pH-adjusted buffered medium, YHI030 strain completely consumed both 50 and 100 g L−1 glucose and, respectively, produced 17.6 and 37.2 g L−1 2,3-BDO (0.36 and 0.38 g g−1 glucose consumed) and glycerol (0.31 and 0.34 g g−1 glucose consumed) (Additional file 1: Figs. S8A and S9A). Fed-batch (consecutive addition) fermentation with 300 g L−1 glucose resulted in essentially complete consumption of the glucose and the production of 81.0 ± 1.3 g L−1 2,3-BDO (at 504 h) (Fig. 10). Although 71.8 ± 0.7 g L−1 glycerol was produced as a major by-product, no ethanol was detected.
In the near future, the subgeneration of abundant glycerol will be decreased by more elaborate control of fermentation conditions than simple aeration and pH, and by genetic modifications such as expression of the noxE gene and deletion of the GPD1 and GPD2 genes, described previously [26, 49]. Other ethanol-reducing yeast strains (e.g., with ADH deletions [26, 50,51,52,53] and various PDC modifications [6, 49, 54]) can also be used to further demonstrate our pyruvate carbon flux tugging strategy, in addition to the PDCΔ strain. Kim et al. recently reported a 2,3-BDO production level of 154.3 g L−1 by S. cerevisiae (fed-batch fermentation) with fine-tuned PDC and noxE activities , and such strains might be compatible for further boosting 2,3-BDO production using our proposed strategy.
In this study, we demonstrated that a strategy for tugging carbon flux can increase 2,3-BDO production and reduce ethanol subgeneration in Crabtree-positive S. cerevisiae. A stronger pulling effect at the hub branching point (tug of carbon flux) was critical in our strategy. Pyruvate was chosen as an example of an important hub compound because it links to both the TCA cycle and amino acid biosynthesis. A high-activity ALS and PDCΔ strain was effective in exerting the pyruvate pulling effect, achieving a high titer of 2,3-BDO and no ethanol subgeneration. This strategy could be used for the production of other chemicals such as isobutanol and 3-methyl-1-butanol (via valine biosynthesis) [55,56,57].
- alsLp :
ALS gene from Lactobacillus plantarum
- alsLpOp :
codon-optimized alsLp gene
- alsTf :
ALS gene from Thermobifida fusca
- alsTfOp :
codon-optimized alsTf gene
coding DNA sequence
- GPD :
glycerol-3-phosphate dehydrogenase gene
high-performance liquid chromatography
Integrative Genomics Viewer
- ILV2c :
the truncated version of the ILV2 gene lacking the mitochondrial signal sequence
- ilvBEc :
ALS gene from Escherichia coli
- ilvBEcOp :
codon-optimized ilvBEc gene
liquid chromatography–tandem mass spectrometry
methyl ethyl ketone (butanone)
- noxE :
NADH oxidase gene
single nucleotide polymorphism
Steensels J, Snoek T, Meersman E, Picca Nicolino M, Voordeckers K, Verstrepen KJ. Improving industrial yeast strains: exploiting natural and artificial diversity. FEMS Microbiol Rev. 2014;38:947–95.
Nishimura Y, Matsui T, Ishii J, Kondo A. Metabolic engineering of the 2-ketobutyrate biosynthetic pathway for 1-propanol production in Saccharomyces cerevisiae. Microb Cell Fact. 2018;17:38.
Steen EJ, Chan R, Prasad N, Myers S, Petzold CJ, Redding A, Ouellet M, Keasling JD. Metabolic engineering of Saccharomyces cerevisiae for the production of n-butanol. Microb Cell Fact. 2008;7:36.
Kondo T, Tezuka H, Ishii J, Matsuda F, Ogino C, Kondo A. Genetic engineering to enhance the Ehrlich pathway and alter carbon flux for increased isobutanol production from glucose by Saccharomyces cerevisiae. J Biotechnol. 2012;159:32–7.
Rao Z, Ma Z, Shen W, Fang H, Zhuge J, Wang X. Engineered Saccharomyces cerevisiae that produces 1,3-propanediol from d-glucose. J Appl Microbiol. 2008;105:1768–76.
Kim SJ, Seo SO, Jin YS, Seo JH. Production of 2,3-butanediol by engineered Saccharomyces cerevisiae. Bioresour Technol. 2013;146:274–81.
Lian JZ, Chao R, Zhao HM. Metabolic engineering of a Saccharomyces cerevisiae strain capable of simultaneously utilizing glucose and galactose to produce enantiopure (2R,3R)-butanediol. Metab Eng. 2014;23:92–9.
Kim SJ, Seo SO, Park YC, Jin YS, Seo JH. Production of 2,3-butanediol from xylose by engineered Saccharomyces cerevisiae. J Biotechnol. 2014;192:376–82.
Nan H, Seo SO, Oh EJ, Seo JH, Cate JHD, Jin YS. 2,3-Butanediol production from cellobiose by engineered Saccharomyces cerevisiae. Appl Microbiol Biotechnol. 2014;98:5757–64.
Bialkowska AM. Strategies for efficient and economical 2,3-butanediol production: new trends in this field. World J Microbiol Biotechnol. 2016;32:200.
Xu Y, Chu H, Gao C, Tao F, Zhou Z, Li K, Li L, Ma C, Xu P. Systematic metabolic engineering of Escherichia coli for high-yield production of fuel bio-chemical 2,3-butanediol. Metab Eng. 2014;23:22–33.
Kim SJ, Kim JW, Lee YG, Park YC, Seo JH. Metabolic engineering of Saccharomyces cerevisiae for 2,3-butanediol production. Appl Microbiol Biotechnol. 2017;101:2241–50.
Song D, Yoon YG, Lee CJ. Conceptual design for the recovery of 1,3-Butadiene and methyl ethyl ketone via a 2,3-Butanediol-dehydration process. Chem Eng Res Des. 2017;123:268–76.
Zheng QX, Wales MD, Heidlage MG, Rezac M, Wang HW, Bossmann SH, Hohn KL. Conversion of 2,3-butanediol to butenes over bifunctional catalysts in a single reactor. J Catal. 2015;330:222–37.
Lynch J. BD monomer and elastomer production processes. Chem Biol Interact. 2001;135:147–53.
Maji T, Mendis CH, Thompson WH, Tunge JA. Evidence for isomerizing hydroformylation of butadiene. A combined experimental and computational study. J Mol Catal A Chem. 2016;424:145–52.
Zellmer L. The 100 most important chemical compounds: a reference guide. Libr J. 2007;132:158.
Stytsenko VD, Mel’nikov DP. Selective hydrogenation of dienic and acetylenic compounds on metal-containing catalysts. Russ J Phys Chem A. 2016;90:932–42.
Ishii J, Tominaga M, Nishida K, Matsuda F, Nishi T, Hasunuma T, Moriya H, Kuriya Y, Araki M, Hara KY, et al. Synthetic bioengineering: a more intensely engineering-conscious sub-discipline of synthetic biology—drawing upon a SynBio toolbox and yeast metabolic engineering. 2018. under revision.
Hagman A, Piskur J. A study on the fundamental mechanism and the evolutionary driving forces behind aerobic fermentation in yeast. PLoS ONE. 2015;10:e0116942.
Kajihata S, Matsuda F, Yoshimi M, Hayakawa K, Furusawa C, Kanda A, Shimizu H. 13C-based metabolic flux analysis of Saccharomyces cerevisiae with a reduced Crabtree effect. J Biosci Bioeng. 2015;120:140–4.
Simeonidis E, Murabito E, Smallbone K, Westerhoff HV. Why does yeast ferment? A flux balance analysis study. Biochem Soc Trans. 2010;38:1225–9.
Vemuri GN, Eiteman MA, McEwen JE, Olsson L, Nielsen J. Increasing NADH oxidation reduces overflow metabolism in Saccharomyces cerevisiae. Proc Natl Acad Sci USA. 2007;104:2402–7.
Matsuda F, Furusawa C, Kondo T, Ishii J, Shimizu H, Kondo A. Engineering strategy of yeast metabolism for higher alcohol production. Microb Cell Fact. 2011;10:70.
Ryan ED, Kohlhaw GB. Subcellular localization of isoleucine-valine biosynthetic enzymes in yeast. J Bacteriol. 1974;120:631–7.
Kim S, Hahn JS. Efficient production of 2,3-butanediol in Saccharomyces cerevisiae by eliminating ethanol and glycerol production and redox rebalancing. Metab Eng. 2015;31:94–101.
Sikorski RS, Hieter P. A system of shuttle vectors and yeast host strains designed for efficient manipulation of DNA in Saccharomyces cerevisiae. Genetics. 1989;122:19–27.
Akada R, Kitagawa T, Kaneko S, Toyonaga D, Ito S, Kakihara Y, Hoshida H, Morimura S, Kondo A, Kida K. PCR-mediated seamless gene deletion and marker recycling in Saccharomyces cerevisiae. Yeast. 2006;23:399–405.
Gietz D, Stjean A, Woods RA, Schiestl RH. Improved method for high-efficiency transformation of intact yeast-cells. Nucleic Acids Res. 1992;20:1425.
Langmead B, Salzberg SL. Fast gapped-read alignment with Bowtie 2. Nat Methods. 2012;9:357–9.
Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N, Marth G, Abecasis G, Durbin R. Genome project data processing S. The sequence alignment/map format and SAMtools. Bioinformatics. 2009;25:2078–9.
Robinson JT, Thorvaldsdottir H, Winckler W, Guttman M, Lander ES, Getz G, Mesirov JP. Integrative genomics viewer. Nat Biotechnol. 2011;29:24–6.
Singh BK, Stidham MA, Shaner DL. Assay of acetohydroxyacid synthase. Anal Biochem. 1988;171:173–9.
Lee YT, Duggleby RG. Mutations in the regulatory subunit of yeast acetohydroxyacid synthase affect its activation by MgATP. Biochem J. 2006;395:331–6.
Nishino S, Okahashi N, Matsuda F, Shimizu H. Absolute quantitation of glycolytic intermediates reveals thermodynamic shifts in Saccharomyces cerevisiae strains lacking PFK1 or ZWF1 genes. J Biosci Bioeng. 2015;120:280–6.
Renna MC, Najimudin N, Winik LR, Zahler SA. Regulation of the Bacillus subtilis alsS, alsD, and alsR genes involved in post-exponential-phase production of acetoin. J Bacteriol. 1993;175:3863–75.
Ishii J, Izawa K, Matsumura S, Wakamura K, Tanino T, Tanaka T, Ogino C, Fukuda H, Kondo A. A simple and immediate method for simultaneously evaluating expression level and plasmid maintenance in yeast. J Biochem. 2009;145:701–8.
Matsuda F, Kondo T, Ida K, Tezuka H, Ishii J, Kondo A. Construction of an artificial pathway for isobutanol biosynthesis in the cytosol of Saccharomyces cerevisiae. Biosci Biotechnol Biochem. 2012;76:2139–41.
Ishii J, Kondo T, Makino H, Ogura A, Matsuda F, Kondo A. Three gene expression vector sets for concurrently expressing multiple genes in Saccharomyces cerevisiae. FEMS Yeast Res. 2014;14:399–411.
Oud B, Flores CL, Gancedo C, Zhang X, Trueheart J, Daran JM, Pronk JT, van Maris AJ. An internal deletion in MTH1 enables growth on glucose of pyruvate-decarboxylase negative, non-fermentative Saccharomyces cerevisiae. Microb Cell Fact. 2012;11:131.
Schneider R, Brors B, Burger F, Camrath S, Weiss H. Two genes of the putative mitochondrial fatty acid synthase in the genome of Saccharomyces cerevisiae. Curr Genet. 1997;32:384–8.
Moriya H, Shimizu-Yoshida Y, Omori A, Iwashita S, Katoh M, Sakai A. Yak1p, a DYRK family kinase, translocates to the nucleus and phosphorylates yeast Pop2p in response to a glucose signal. Genes Dev. 2001;15:1217–28.
Garrett S, Menold MM, Broach JR. The Saccharomyces cerevisiae YAK1 gene encodes a protein kinase that is induced by arrest early in the cell cycle. Mol Cell Biol. 1991;11:4045–52.
Colombie S, Dequin S, Sablayrolles JM. Control of lactate production by Saccharomyces cerevisiae expressing a bacterial LDH gene. Enzyme Microbial Technol. 2003;33:38–46.
Cordova LT, Alper HS. Central metabolic nodes for diverse biochemical production. Curr Opin Chem Biol. 2016;35:37–42.
van Maris AJ, Geertman JM, Vermeulen A, Groothuizen MK, Winkler AA, Piper MD, van Dijken JP, Pronk JT. Directed evolution of pyruvate decarboxylase-negative Saccharomyces cerevisiae, yielding a C2-independent, glucose-tolerant, and pyruvate-hyperproducing yeast. Appl Environ Microbiol. 2004;70:159–66.
Flikweert MT, Van Der Zanden L, Janssen WM, Steensma HY, Van Dijken JP, Pronk JT. Pyruvate decarboxylase: an indispensable enzyme for growth of Saccharomyces cerevisiae on glucose. Yeast. 1996;12:247–57.
Flikweert MT, de Swaaf M, van Dijken JP, Pronk JT. Growth requirements of pyruvate-decarboxylase-negative Saccharomyces cerevisiae. FEMS Microbiol Lett. 1999;174:73–9.
Kim JW, Seo SO, Zhang GC, Jin YS, Seo JH. Expression of Lactococcus lactis NADH oxidase increases 2,3-butanediol production in Pdc-deficient Saccharomyces cerevisiae. Bioresour Technol. 2015;191:512–9.
Ida Y, Furusawa C, Hirasawa T, Shimizu H. Stable disruption of ethanol production by deletion of the genes encoding alcohol dehydrogenase isozymes in Saccharomyces cerevisiae. J Biosci Bioeng. 2012;113:192–5.
Ida Y, Hirasawa T, Furusawa C, Shimizu H. Utilization of Saccharomyces cerevisiae recombinant strain incapable of both ethanol and glycerol biosynthesis for anaerobic bioproduction. Appl Microbiol Biotechnol. 2013;97:4811–9.
Hirasawa T, Ida Y, Furusawa C, Shimizu H. Potential of a Saccharomyces cerevisiae recombinant strain lacking ethanol and glycerol biosynthesis pathways in efficient anaerobic bioproduction. Bioengineered. 2014;5:123–8.
Tokuhiro K, Ishida N, Nagamori E, Saitoh S, Onishi T, Kondo A, Takahashi H. Double mutation of the PDC1 and ADH1 genes improves lactate production in the yeast Saccharomyces cerevisiae expressing the bovine lactate dehydrogenase gene. Appl Microbiol Biotechnol. 2009;82:883–90.
Kim JW, Kim J, Seo SO, Kim KH, Jin YS, Seo JH. Enhanced production of 2,3-butanediol by engineered Saccharomyces cerevisiae through fine-tuning of pyruvate decarboxylase and NADH oxidase activities. Biotechnol Biofuels. 2016;9:265.
Atsumi S, Hanai T, Liao JC. Non-fermentative pathways for synthesis of branched-chain higher alcohols as biofuels. Nature. 2008;451:86–9.
Matsuda F, Ishii J, Kondo T, Ida K, Tezuka H, Kondo A. Increased isobutanol production in Saccharomyces cerevisiae by eliminating competing pathways and resolving cofactor imbalance. Microb Cell Fact. 2013;12:119.
Park SH, Kim S, Hahn JS. Metabolic engineering of Saccharomyces cerevisiae for the production of isobutanol and 3-methyl-1-butanol. Appl Microbiol Biotechnol. 2014;98:9139–47.
JI and FM designed the research. JI, KM, KI, HK, SH and FM performed the experiments and analyzed data. SK acquired the metabolome data. KM carried out sample preparation and data analysis for genome re-sequencing. JI, HS and FM interpreted the data. JI and FM wrote the manuscript. JI, KI and FM participated in conception of the study. JI, HS, AK, and FM co-coordinated this research project. All authors read and approved the final manuscript.
Data acquisition by the next-generation sequencer was supported by Prof. Yuu Hirose (Toyohashi University of Technology, Japan). Plasmid vectors (pGK425 and pAT425) were provided by the National Bio-Resource Project (NBRP), Japan.
The authors declare that they have no competing interests.
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This work was supported by the Industrial Technology Research Grant Program for 2011 of the New Energy and Industrial Technology Development Organization (NEDO); a Grant-in-Aid for Scientific Research (C) no. 15K06579 and 18K04851; a JST-Mirai Program Grant Number JPMJMI17EJ; and the Special Coordination Funds for Promoting Science and Technology, Creation of Innovation Centers for Advanced Interdisciplinary Research Areas (Innovative Bioproduction Kobe; iBioK) from the Ministry of Education, Culture, Sports, Science and Technology (MEXT) of Japan.
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About this article
- Pyruvate flux
- Crabtree effect
- Acetolactate synthase
- Ethanol subgeneration
- 2,3-Butanediol production
- Pyruvate decarboxylase (PDC) deficient