Skip to main content
Download PDF

A highly efficient transcriptome-based biosynthesis of non-ethanol chemicals in Crabtree negative Saccharomyces cerevisiae

Biotechnology for Biofuels and Bioproducts volume 16, Article number: 37 (2023) Cite this article

Abstract

Background

Owing to the Crabtree effect, Saccharomyces cerevisiae produces a large amount of ethanol in the presence of oxygen and excess glucose, leading to a loss of carbon for the biosynthesis of non-ethanol chemicals. In the present study, the potential of a newly constructed Crabtree negative S. cerevisiae, as a chassis cell, was explored for the biosynthesis of various non-ethanol compounds.

Results

To understand the metabolic characteristics of Crabtree negative S. cerevisiae sZJD-28, its transcriptional profile was compared with that of Crabtree positive S. cerevisiae CEN.PK113-11C. The reporter GO term analysis showed that, in sZJD-28, genes associated with translational processes were down-regulated, while those related to carbon metabolism were significantly up-regulated. To verify a potential increase in carbon metabolism for the Crabtree negative strain, the production of non-ethanol chemicals, derived from different metabolic nodes, was then undertaken for both sZJD-28 and CEN.PK113-11C. At the pyruvate node, production of 2,3-butanediol and lactate in sZJD-28-based strains was remarkably higher than that of CEN.PK113-11C-based ones, representing 16.8- and 1.65-fold increase in titer, as well as 4.5-fold and 0.65-fold increase in specific titer (mg/L/OD), respectively. Similarly, for shikimate derived p-coumaric acid, the titer of sZJD-28-based strain was 0.68-fold higher than for CEN.PK113-11C-based one, with a 0.98-fold increase in specific titer. While farnesene and lycopene, two acetoacetyl-CoA derivatives, showed 0.21- and 1.88-fold increases in titer, respectively. From malonyl-CoA, the titer of 3-hydroxypropionate and fatty acids in sZJD-28-based strains were 0.19- and 0.76-fold higher than that of CEN.PK113-11C-based ones, respectively. In fact, yields of products also improved by the same fold due to the absence of residual glucose. Fed-batch fermentation further showed that the titer of free fatty acids in sZJD-28-based strain 28-FFA-E reached 6295.6 mg/L with a highest reported specific titer of 247.7 mg/L/OD in S. cerevisiae.

Conclusions

Compared with CEN.PK113-11C, the Crabtree negative sZJD-28 strain displayed a significantly different transcriptional profile and obvious advantages in the biosynthesis of non-ethanol chemicals due to redirected carbon and energy sources towards metabolite biosynthesis. The findings, therefore, suggest that a Crabtree negative S. cerevisiae strain could be a promising chassis cell for the biosynthesis of various chemicals.

Background

With growing concern regarding environmental protection and energy security, microbial productions of biobased chemicals are getting increasing attention. Among them, Saccharomyces cerevisiae is a widely used model organism due to its advantages of well-understood genetic background, feasible molecular manipulation and high robustness to industrial conditions [1,2,3,4]. However, the ethanol overflow metabolism of S. cerevisiae, also referred to as the Crabtree effect, causes considerable loss of carbon flux in the production of non-ethanol chemicals [5].

Attempts to delete ethanol biosynthetic pathway have been, therefore, made to achieve Crabtree negative S. cerevisiae to eliminate the carbon loss, and in this context, since alcohol dehydrogenase (ADH) converts aldehyde into ethanol, deletion of all ADH isozymes has been envisaged as a potential solution [6]. However, ADH activity is required for the synthesis of many other specific metabolites, e.g., higher alcohols [7]. At the same time, pyruvate decarboxylase, encoded by PDC, converts pyruvate to aldehyde in the cytoplasm, followed by conversion to acetate, i.e., the precursor of acetyl-CoA. Hence, even though inactivation of PDCs genes enables redirection of metabolic flux from ethanol towards the productions of target chemicals [8], Pdc− strains are notoriously known for inability to grow in the presence of excess glucose medium due to inadequate supply of acetyl-CoA as well as NAD+ regeneration. Furthermore, although adaptive laboratory evolution (ALE) [9] and internal deletion in a transcriptional regulator MTH1 [10] relieved the above growth defect of Pdc− strains in glucose-containing medium, the lag phase was 3 days longer and the max specific growth rates were only 0.1 h−1, thus impeding the strains’ industrial applications for biosynthesis.

To increase the availability of cytoplasmic acetyl-CoA for Pdc− strains, pyruvate dehydrogenase complex (PDH), responsible for acetyl-CoA synthesis in mitochondria, was relocated to the cytoplasm [11]. However, the specific growth rate remained low due to PDH’s complex need for cofactors, one of which (lipoic acid) was absent in the cytoplasm. Consequently, the Pdc− strains require a more efficient pathway for supplying acetyl-CoA. Recently, a heterogeneous pathway involving pyruvate oxidase (PO)/phosphotransacetylase (PTA) was used to replace the native PDCs, constructing a Crabtree-negative S. cerevisiae with alternative acetyl-CoA supplying pathway. In addition, double deletions of glycerol 3-phosphate phosphatase (GPP1, GPP2) decreased the accumulation of acetate. Finally, using ALE and reverse engineering conferred the Pdc− strain with two genetic mutations, namely, GPD1W71* and MED2*432Y, forming strain sZJD-28 (Table 1). This strain sZJD-28 produced no ethanol and most carbon source was distributed to biomass and CO2 with growth rate reaching at 0.228 h−1 in glucose medium [12]. To our knowledge, sZJD-28 is the fastest growing Crabtree negative S. cerevisiae, with great prospects in industrial biotechnology. However, the comparison of transcriptional patterns between Crabtree negative sZJD-28 and Crabtree positive yeast has not been demonstrated, with the former’s biosynthesis capacity also being unclear.

Table 1 Strains list in this study
Full size table

In the present study, analysis of Crabtree negative yeast sZJD-28 showed global transcriptional differences related to Crabtree positive strain CEN.PK113-11C, including enhanced carbon metabolism processes and down-regulated protein translation processes. To prove the increased metabolic fluxes towards biosynthesis, non-ethanol products derived from four representative metabolic nodes including pyruvate, malonyl-CoA, acetoacetyl-CoA and shikimate were also tested for both strains. The results highlighted obvious advantages of sZJD-28 in terms of the titer, yield and specific titer of the non-ethanol chemicals. Overall, the results suggested that, as a novel chassis cell, a Crabtree negative S. cerevisiae holds great potential for biomanufacturing of various chemicals.

Results and discussion

Transcriptional comparison between Crabtree negative and positive S. cerevisiae

To elucidate the mechanisms underlying the physiological differences between Crabtree positive and negative S. cerevisiae, the transcriptional profiles of sZJD-28 were compared with that of CEN.PK113-11C using the reporter Gene Ontology (GO) term analysis [13]. Results showed that genes associated with GO terms related to protein translation processes, such as ribosome biogenesis and assembly, rRNA processing, cytoplasmic translation, translational initiation, transcription from RNA polymerase I and II promoter, chromatin organization and mitotic cell cycle, were down-regulated in sZJD-28 (Fig. 1a). In addition, compared with the faster growing CEN.PK113-11C, the transcriptome changes related to the ribosome bioprocess of sZJD-28 further confirmed the growth law that ribosomal protein fraction are related to growth rate [14].

Fig. 1
figure 1figure 1

Transcriptional analysis of sZJD-28 and CEN.PK113-11C. a Gene sets with significant differences in sZJD-28 compared with CEN.PK113-11C. GO terms are colored according to their ranking, and each cell of the heatmap includes the significance of the GO terms. Dist (dn) is distinct-directional down, representing this gene set is coordinately down-regulated. Dist (up) is distinct-directional up, representing this gene set is coordinately up-regulated. Mix (dn) is mixed directional down and Mix (up) is mix-directional up, separately providing the significance of subsets of up- and downregulated genes in a gene set. Nondir is non-directional change, providing gene set p values obtained by omitting the direction of differential expression [13]. b Transcriptional level of genes related to oxidative phosphorylation (OXPHOS) in sZJD-28 compared with CEN.PK113-11C. c Schematic representation of the differential transcriptional changes of genes involved in the glycolysis, tricarboxylic acid (TCA) cycle, mevalonate (MVA) pathway, pentose phosphate pathway (PPP), fatty acid synthesis and shikimate pathway. Color keys demonstrate transcriptional fold changes in sZJD-28 relative to CEN.PK113-11C

Full size image

On the other hand, genes associated with GO terms related to cellular intermediates metabolism were up-regulated in sZJD-28. In particular, the up-regulation of genes related to cellular respiration, lipid, cofactor and carbohydrate metabolic processes, metabolites and energy generation, as well as transmembrane transport-related genes (Fig. 1a), hinted at an increase in the carbon metabolic capacity of Crabtree negative sZJD-28. Meanwhile, strengthened carbon metabolism may also cause stress responses due to the accumulation of intermediates, and this was revealed by up-regulated stress-responsive genes (Fig. 1a). Agreement with this observation, results of reporter transcriptional factors (TFs) analysis highlighted the significantly altered expression of stress-responsive TFs, such as HSF1, YAP1, MSN2, CST6, MSN4 in sZJD-28 compared with CEN.PK113-11C (Additional file 1: Fig. S1).

The central carbon and energy metabolism which were significantly changed at transcriptional levels are described in Fig. 1b, c. In an overall view, glycolysis in sZJD-28 was down-regulated, while PP pathway, TCA cycle and oxidative phosphorylation (OXPHOS) were up-regulated, hence indicating that sZJD-28 might redirect more metabolic flux from fermentation to respiration compared with CEN.PK113-11C. These transcriptional changes also correlated well with the observed difference in growth rates between the two strains as the lower ATP generation rate through respiration instead of glycolysis resulted in a lower growth rate [15]. Besides, sZJD-28 showed increased transcriptional levels of many other metabolic pathways, such as mevalonate pathway, shikimate pathway, fatty acid biosynthesis and β-oxidation pathway. Altogether, these results indicated that Crabtree negative sZJD-28 redistributes the carbon and electron fluxes to strengthen carbon metabolism. These transcriptional changes in Crabtree negative sZJD-28 may further imply an elevated biosynthesis capacity compared with Crabtree positive CEN.PK113-11C when growing in the presence of excess glucose.

Evaluating the capacity of Crabtree negative S. cerevisiae to produce non-ethanol chemicals

The transcriptional levels of genes related to OXPHOS were significantly improved in sZJD-28 compared with CEN.PK113-11C (Fig. 1b), indicating that the cytoplasmic NAD+ regeneration in Crabtree negative S. cerevisiae may be restrained due to the abolished ethanol generation. Thus, an NADH-consuming pathway might relieve the pressure of redox imbalance in sZJD-28.

On the other hand, capacity of biosynthetic pathways with many genes up-regulated might be increased as well. For example, up-regulations of transcriptional levels were generally occurred in PPP, shikimate pathway, MVA pathway and fatty acids pathways. Although some genes in PPP and shikimate pathway were down-regulated, such as ZWF1 and ARO7, the numbers of up-regulated genes were clearly larger than the down-regulated ones. In addition, it is different to confirm the capacity of whole pathway by specific gene’ transcriptional level. This necessitates the demonstration of capacities for different pathways with many up-regulated genes. To confirm the possible enhanced biosynthetic capacity of sZJD-28, different pathways were constructed, based on the transcriptome analysis of both CEN.PK113-11C and sZJD-28, to detect generation of products from four representative metabolic nodes.

Biosynthesis of 2,3-butanediol and lactate from pyruvate

The production of pyruvate-derived, NADH-dependent 2,3-butanediol (2,3-BD) and lactate were first compared in sZJD-28 and CEN.PK113-11C. S. cerevisiae possesses an inherent pathway for generating 2,3-BD from pyruvate (Fig. 2a). As previously reported, an overexpression of acetolactate synthase (ILV2) is sufficient for the production of detectable level of 2,3-BD in S. cerevisiae [16]. Therefore, plasmid-based ILV2 expression was adapted to test the capacity of sZJD-28 and CEN.PK113-11C to produce this compound. It was observed that strain 28-BD, harboring empty plasmid, already produced 208.4 mg/L of 2,3-BD, which was higher than the titer of strain 11C-BD by more than 13 folds, while the specific titer (g/L/OD) was improved by 16.8 folds (Fig. 2b). The yield of 28-BD was also more than 13 folds higher than that of 11C-BD as there was no residual glucose. In addition, the titer of 2,3-BD in ILV2 overexpression strain 28-BD-E was increased to 292.3 mg/L, higher than that of strain 11C-BD-E by over threefolds (Fig. 2b), while the specific titer of 2,3-BD for 28-BD-E was 4.5 folds higher compared with 11C-BD-E (Fig. 2c). These results indicated that the imbalanced NADH level may drive the production of NADH dependent chemicals, such as 2,3-BD, although the transcriptional level of ILV2 was similar between sZJD-28 and CEN.PK113-11C (Additional file 1: Fig. S2). Compared with Crabtree positive strain with different background, such as BY4742, 28-BD also shows fourfold higher yield of 2,3-BD (0.010 vs 0.002 g/g glucose) [17].

Fig. 2
figure 2

Production of 2,3-BD and lactate by Crabtree positive and negative S. cerevisiae. a Schematic representation of 2,3-BD and lactate biosynthetic pathways in S. cerevisiae. Both lactate dehydrogenase (LlLDH) from Lactococcus lactis and cytoplasm-relocated acetolactate synthase (cytoILV2) are shown in red, and yeast native steps, including spontaneous reaction and NAD-dependent (R,R)-butanediol dehydrogenase (BDH1) are shown in orange. b Titer of 2,3-BD produced by Crabtree positive 11C-BD and Crabtree negative 28-BD; c specific titer of 2,3-BD in Crabtree positive 11C-BD and Crabtree negative 28-BD; d titer of lactate produced by Crabtree positive 11C-LA and Crabtree negative 28-LA; e specific titer of lactate in Crabtree positive 11C-LA and Crabtree negative 28-LA. **p value < 0.005, *p value < 0.05

Full size image

Lactate is another NADH-dependent chemical derived from pyruvate (Fig. 2a). However, S. cerevisiae lacks a native lactate dehydrogenase (LDH) for lactate production, but it contains a mitochondrial LDHs (CYB2 and DLD1) that convert lactate to pyruvate. To test the potential advantage on cytosolic NADH provision of sZJD-28, an NADH-dependent LDH from Lactococcus lactis was introduced into CEN.PK113-11C and sZJD-28, resulting in strains 11C-LA and 28-LA, respectively. The results showed that 3.18 g/L of lactate was accumulated by 28-LA, while strain 11C-LA produced lactate with a peak value at 1.16 g/L. However, the latter consumed the lactate when glucose was exhausted (Fig. 2d, Additional file 1: Fig. S3). At the same time, the maximal specific titer of 28-LA was 64.9% higher than that of 11C-LA (Fig. 2e).

In S. cerevisiae, CYB2 and DLD1 are two genes involved in lactate utilization, whose expression are repressed by glucose and derepressed in ethanol or lactate [18, 19]. In sZJD-28, the transcriptional level of CYB2 was increased by 1.3-fold, while the transcriptional level of DLD1 was only decreased by 17% (Additional file 1: Fig. S2). With the significant decreased transcriptional levels of low-affinity glucose transporters HXT1 and HXT3 compared with CEN.PK113-11C (Additional file 1: Fig. S2), glucose repression could have been partially relieved in sZJD-28, resulting in the improved transcriptional level of CYB2. Strain 28-LA accumulated lactate instead of consuming it as it was the case for 11C-LA, demonstrating the dominant role of NADH consumption in Crabtree negative strain sZJD-28. Overall, the above results indicated that sZJD-28 possessed more efficient pyruvate and NADH supply compared with CEN.PK113-11C. In addition, lactate production of Crabtree positive strain CEN.PK2-1C harboring different LDHs reached a maximal titer of 2.50 g/L [20], lower than that of 28-LA (3.18 g/L).

p-Coumaric acid biosynthesis from shikimate pathway

The shikimate pathway is usually applied in the synthesis of aromatic amino acids (AAAs) and their derivatives (AAADs) which serve as precursors for various industrially relevant compounds [21]. For overproduction of shikimate derivatives in S. cerevisiae, enhancing the expression of native genes such as ARO1-4 and ARO7-9 is the common metabolic engineering strategy [22,23,24,25,26,27]. As shown in Fig. 1c, increased transcriptional level of phenylalanine and tyrosine biosynthesis such as the ARO genes and their precursor biosynthesis pathway PPP were observed for sZJD-28 compared with CEN.PK113-11C. Furthermore, Pdc5p consume precursors of AAAs, para-hydroxy-phenylpyruvate and phenylpyruvate into fusel alcohol/acid [28]. The deficiency of Pdc5p sZJD-28 may be advantageous for the biosynthesis of AAAs and AAADs. These results indicated that sZJD-28 could be a superior strain for synthesizing aromatic chemicals compared with CEN.PK113-11C.

To confirm the above hypothesis, p-coumaric acid was selected as a representative AAAD for subsequent experiments. The tyrosine ammonia lyase (FjTAL) from Flavobacterium johnsoniae, which could covert tyrosine into p-coumaric acid, was expressed in sZJD-28 and CEN.PK113-11C resulting in 28-PCA and 11C-PCA, respectively (Fig. 3a). The production of p-coumaric acid by 28-PCA reached 270.7 mg/L, which was 67.8% higher than that of 11C-PCA (Fig. 3b), and the yield was also 67.8% higher than that of 11C-PCA due to no detected residual glucose. The specific titer in 28-PCA was increased by 97.5% than that of 11C-PCA (Fig. 3c). These results proved that the Crabtree negative S. cerevisiae sZJD-28 could display enhanced capacity for AAADs biosynthesis compared with the Crabtree positive S. cerevisiae CEN.PK113-11C. For other Crabtree positive S. cerevisiae, CEN.PK102.5B and BY4741-based p-coumaric acid producers reached titers of 0.202 and 0.081 g/L [29], which were lower than that of 28-PCA (Fig. 3b).

Fig. 3
figure 3

Production of p-coumaric acid by Crabtree positive and negative S. cerevisiae. a Schematic representation of p-coumaric acid biosynthetic pathways in S. cerevisiae. Yeast native genes, including pentafunctional arom protein (ARO1), bifunctional chorismate synthase/riboflavin reductase (ARO2), 3-deoxy-7-phosphoheptulonate synthase (ARO3, ARO4), chorismate mutase (ARO7), aromatic aminotransferase I (ARO8), aromatic aminotransferase II (ARO9), and prephenate dehydrogenase (TYR1) are shown in orange. Tyrosine ammonia lyase (FjTAL) from Flavobacterium johnsoniae is shown in red. b Titer of p-coumaric acid produced by Crabtree positive 11C-PCA and Crabtree negative 28-PCA; c specific titer of p-coumaric acid in Crabtree positive 11C-PCA and Crabtree negative 28-PCA. *p value < 0.05

Full size image

Farnesene and lycopene biosynthesis from acetoacetyl-CoA

The MVA pathway is usually used by S. cerevisiae to synthesize isoprenoids [30, 31]. In sZJD-28, the transcriptional level of this pathway was clearly higher than that of CEN.PK113-11C (Fig. 1c). Acetyl-CoA C-acetyltransferase (Erg10p) serves as the first enzyme in the MVA pathway [32], whereas HMG-CoA reductase (Hmg2p) [33] and isopentenyl pyrophosphate isomerase (Idi1p) [34] play rate-limiting roles in sterol biosynthesis. Mevalonate pyrophosphate decarboxylase (Mvd1p) [35], farnesyl pyrophosphate synthetase (Erg20p) [36] and geranylgeranyl diphosphate synthase (Bts1p) [37] serve as essential enzymes involved in the biosynthesis of isoprenoids (Fig. 4a). Increasing the transcription levels of these genes in S. cerevisiae have already been proven to improve the production of isoprenoids [38,39,40,41,42].

Fig. 4
figure 4

Production of farnesene and lycopene by Crabtree positive and negative S. cerevisiae. a Schematic representation of farenese and lycopene biosynthetic pathways in S. cerevisiae. Yeast native genes including phosphomevalonate kinase (ERG8), acetyl-CoA C-acetyltransferase (ERG10), mevalonate kinase (ERG12), 3-hydroxy-3-methylglutaryl-CoA (HMG-CoA) synthase (ERG13), farnesyl pyrophosphate synthetase (ERG20), HMG-CoA reductase (HMG1, HMG2), isopentenyl diphosphate: dimethylallyl diphosphate isomerase (IDI1), mevalonate pyrophosphate decarboxylase (MVD1), and geranylgeranyl diphosphate synthase (BTS1) are shown in orange. Farnesene synthase (MdFS) from Malus domestica, geranylgeranyl pyrophosphate synthase (PaCrtE) from Pantoea ananatis, phytoene synthase (PaCrtB) from Pantoea ananatis, and phytoene desaturase (PaCrtI) from Pantoea ananatis are shown in red. b Titer of farnesene produced by Crabtree positive 11C-Far and 28-Far. c Titer of lycopene produced by Crabtree positive 11C-Lyc and Crabtree negative 28-Lyc. *p value < 0.05

Full size image

To demonstrate the potential strength of sZJD-28 on isoprenoids biosynthesis, two representative isoprenoids, namely, farnesene and lycopene, were selected. Overexpression of farnesene synthase rendered farnesene production in both sZJD-28 and CEN.PK113-11C, resulting in strains 28-Far and 11C-Far. The titer of farnesene in strain 28-Far was 20.5% higher than that of strain 11-Far (Fig. 4b). Crabtree positive strain YPH499 with farnesene synthase produced farnesene in titer of approximate 12.5 mg/L [43], lower than that of 28-Far (Fig. 4b). Similarly, after introducing CrtE, CrtB and CrtI, the three genes encoding key enzymes for lycopene biosynthesis, into the sZJD-28 and CEN.PK113-11C, the lycopene production of strain 28-Lyc reached 34.4 mg/L which was 1.88 times greater than that of strain 11-Lyc (Fig. 4c). The improvements in the yields of farnesene and lycopene are the same as the final titers as there was not detected any residual glucose. Overall, the biosynthetic capacity of isoprenoids with acetoacetyl-CoA as precursor was stronger in Crabtree negative sZJD-28 compared with Crabtree negative CEN.PK113-11C. Specific titer of 28-Lyc reached 13.51 mg/g DCW, which was much higher than those of lycopene-producers derived from Crabtree positive strains, such as CEN.PK2-1D (approximate 5 mg/g DCW) [44] and BY4741 (approximate 4 mg/g DCW) [45].

3-Hydroxypropionic acid and free fatty acids biosynthesis from malonyl-CoA

In addition to the above metabolic nodes, malonyl-CoA is also an important precursor for chemical biosynthesis (Fig. 5a). In this case, the transcriptional analysis indicated that malonyl-CoA derived fatty acid metabolism in sZJD-28 was more active compared with CEN.PK113-11C (Fig. 1c). In particular, the transcriptional level of ACC1, involved in the generation of malonyl-CoA in sZJD-28, was 74.8% higher than in CEN.PK113-11C (Additional file 1: Fig. S4).

Fig. 5
figure 5

Production of 3-HP and free fatty acids by Crabtree positive and negative S. cerevisiae. a Schematic representation of 3-HP and free fatty acids biosynthetic pathway in S. cerevisiae. Yeast native genes, including acetyl-CoA carboxylase (ACC1), beta subunit of fatty acid synthetase (FAS1), alpha subunit of fatty acid synthetase (FAS2), peroxisomal acyl-CoA thioesterase (TES1), long chain fatty acyl-CoA synthetase (FAA1, FAA4), and fatty-acyl coenzyme A oxidase (POX1) are shown in orange. Malonyl-CoA reductase (CaMCR) from Chloroflexus aurantiacus is shown in red. b Titer of 3-HP produced by Crabtree positive 11C-HP and negative 28-HP; c Specific titer of 3-HP in Crabtree positive 11C-HP and negative 28-HP; c titer of FFA produced by Crabtree positive 11C-FFA, negative 28-FFA and 28-FFA-E; d specific titer of FFA in Crabtree positive 11C-FFA, negative 28-FFA and 28-FFA-E. ***p value < 0.001; **p value < 0.005; *p value < 0.05

Full size image

To confirm these results, 3-hydroxypropionic acid and free fatty acids, the malonyl-CoA derivatives, were selected to determine the potential advantage of sZJD-28. The resulting strains 11C-HP and 28-HP were obtained after heterologous expression of malonyl-CoA reductase (MCR1) from Chloroflexus aurantiacus in CEN.PK113-11C and sZJD-28. As expected, 3-HP production in 28-HP was 19.2% higher than in 11C-HP (Fig. 5b), and the specific titer was 20.8% higher (Fig. 5c). In addition, compared with a reported study about the production the 3-HP by Crabtree positive strains, sZJD-28 also showed a 4.57-fold higher titer [46], also indicating the higher biosynthetic capacity of Crabtree negative strains. As previously reported, simultaneously deleting FAA1, FAA4 and POX1 enabled S. cerevisiae to accumulate free fatty acids (FFA) [47]. Therefore, these three genes were deleted in sZJD-28 and CEN.PK113-11C, resulting in strains 28-FFA and 11C-FFA. Compared with 11C-FFA, 28-FFA showed higher production of free fatty acids by 76.3%, reaching 780.4 mg/L (Fig. 5c) and higher specific titer by 71.5% (Fig. 5d). The improvements in yields of 3-HP and FAA also reached 19.2% and 76.3% as no residual glucose. Besides the key gene ACC1, the up-regulated FAS1 and FAS2 (Additional file 1: Fig. S2) could also have contributed to the improved capacity for fatty acids biosynthesis of sZJD-28.

Compared with Crabtree positive strains, Crabtree negative ones showed superior biosynthetic capabilities for chemicals derived from multiple metabolic nodes. Of these, lactate and 2,3-BD derived from pyruvate were significantly improved, while p-coumaric acid derived from shikimate, 3-HP derived from malonyl-CoA, and farnesene derived from acetoacetyl-CoA showed modest improvements in the Crabtree negative strain. This was probably due to needs for different cofactors for different pathways. Ethanol production consumes the surplus NADH generated by glycolysis, such that deleting ethanol synthesis leads to accumulation of NADH in the Crabtree negative strain. The biosynthesis of 2,3-BD and lactate requires the use of the cofactor NADH and this ensures a balance of NADH production in the cytosol during the conversion of glucose to pyruvate [48, 49]. In the shikimate pathway, NAD+ instead of NADH is needed for Pha2p and Try1p, and hence, a similar balance in NADH is not achieved when using this pathway. MCR1 from Chloroflexus aurantiacus [50] used for the production of 3-HP and over-expression of HMGR [51] in the MVA pathway are both NADPH-dependent. Consequently, for these products there was no balancing of NADH. The different cofactors needed for producing the different products may, therefore, result in varying performance during improving biosynthesis by the Crabtree negative chassis strain.

Fed-batch fermentation of Crabtree negative FFA hyperproducing S. cerevisiae

As reported, deleting PAH1 could stimulate FFA production in the Crabtree positive S. cerevisiae due to the up-regulation of fatty acid biosynthesis indirectly by phosphatidic acid [47]. To construct a Crabtree negative FFA hyperproducer, PAH1 was, therefore, deleted based on strain 28-FFA. The resulting strain 28-FFA-E showed 75.3% and 86.7% higher FFA titer and specific titer, respectively, compared with 28-FFA. reaching 1333.2 mg/L and 217.7 mg/L/OD (Fig. 5e). To investigate the biosynthetic capacity of this FFA producer, fed-batch fermentation of 28-FFA-E was conducted in a 5 L bioreactor. During the fermentation process, glucose consumption, cell growth as well as production of FFA and intermediates were monitored. Glucose feeding was initiated at 40 h and glucose concentration was kept below 1 g/L. KOH was used to adjust pH to 5.0 and the dissolved oxygen was maintained above 20% by automatic adjustment of stirring rate. After 180 h, the titer of FFA reached 6295.6 mg/L (Fig. 6a).

Fig. 6
figure 6

Fed-batch fermentation of FFA in 28-FFA-E. Cultivation was carried out in minimal salt medium with pH 5.0 adjusted by KOH. The dissolved oxygen concentration was maintained above 20% saturation by automatic adjustment of the stirring rate. Glucose feeding was initiated at 40 h. a FFA production, OD and glucose consumption by Crabtree negative 28-FFA-E. FFA titer is the sum of all detected FFA, including C8, C10, C12, C14, C16:1, C16, C18, C18:1; b production of pyruvate and citrate during fed-batch fermentation of FFA in Crabtree negative 28-FFA-E

Full size image

Although fed-batch production of FFA was lower than the highest titer reported for a Crabtree positive S. cerevisiae strain, i.e., Y&Z036 (33.4 g/L) [52], the specific titer of 28-FFA-E reached 247.7 mg/L/OD which is over 2 folds higher than that of Y&Z036. In addition, the FFA content of 28-FFA-E reached 897.3 mg/g DCW (according to 3.55 OD = 1 g DCW/L [53]), and as such it was comparable with the content of oleaginous yeast Yarrowia lipolytica (1200 mg/g DCW) [54] and higher than the specific titer of E. coli (about 470 mg/g DCW) [55] according to 1 OD = 0.379 g DCW/L [56]. It is worth noting that specific titers reached close to and higher than the 1000 mg/g DCW due to the secretion of fatty acids into the culture broth. Despite of the lower FFA titer of 28-FFA-E than the Crabtree positive S. cerevisiae strain Y&Z036 [52], 28-FFA-E still showed great potential in FFA biosynthesis, because there was much less genetic optimization performed in 28-FFA-E. Furthermore, as shown in Fig. 6b, the high accumulation of pyruvate and citrate in the fed-batch fermentation process, reached 27.8 g/L and 5.2 g/L, respectively, thereby causing carbon loss and low biomass. To overcome these problems, increasing the copy of PO-PTA and heterogenous expression of ATP-citrate lyase, converting pyruvate and citrate to acetyl-CoA, respectively, could relieve intermediates accumulations, thus resulting in more carbon towards the biosynthesis of targeted chemicals.

Conclusions

In this study, comparative transcriptome analysis between Crabtree positive and the fast-growing Crabtree negative S. cerevisiae was demonstrated for the first time. It turned out that transcriptional levels of genes related to OXPHOS and central metabolic pathways were changed significantly. This analysis provided key information about the potential pathways for non-ethanol chemicals production, which is helpful to choose chemicals synthesized in this superior chassis cell. The following demonstration of productions from various metabolic nodes confirmed the advantages of Crabtree negative strains in yield, titer and specific titer. In addition, this study collectively showed the preferable feature of Crabtree negative strains in NADH-consuming chemicals biosynthesis by balancing redox homeostasis. Among these chemicals, compared with Crabtree positive strain, productions of NADH dependent chemicals 2,3-BD and lactate in Crabtree negative strains were significantly improved by 16.8 and 1.65 folds in titers, respectively; Productions of p-coumaric acid, farnesene, lycopene, 3-HP and FFA from corresponding pathways with up-regulated genes in Crabtree negative strains were improved by 0.19–1.88-folds in titer; In fed-batch, Crabtree negative 28-FFA-E reached a highest reported specific titer of FFA in S. cerevisiae. This research not only deepened the current understanding of the carbon metabolism of Crabtree negative S. cerevisiae, but also proved that such a strain possesses inherent superiority for chemicals biosynthesis, thereby providing an alternative chassis cell for synthetic biology.

Methods

Culture conditions and media

Escherichia coli DH5a was routinely used for plasmid propagation in LB medium, consisting of 10 g/L tryptone, 5 g/L yeast extract and 10 g/L NaCl.

Saccharomyces cerevisiae harboring different biosynthetic pathways was transferred from glycerol stock to 5 mL minimal medium, consisting of the following components: 20 g/L glucose, 14.4 g/L KH2PO4, 7.5 g/L (NH4)2SO4, 0.5 g/L MgSO4·7H2O, trace metal, vitamin solution, 40 mg/L histidine and/or 40 mg/L uracil according to auxotroph [57]. Transfer the culture to 20 mL same medium with initial OD of 0.05 when strains were grown to log-phase, and fermentation broth were sampled for analysis at 120 h. For CEN.PK113-11C and sZJD-28 derived strains, samples were taken between 0 and 120 h, which is longer enough to consume carbon source and suitable for evaluate the biosynthetic capacity of chemicals.

Transcriptome analysis

Glycerol stocks of sZJD-28 and CEN.PK113-11C were transferred into 5 mL YPD (20 g/L glucose, 20 g/L peptone and 10 g/L yeast extract) medium, and incubated at 30 °C, 250 rpm for 24 h. Cells were harvested by centrifuging at 12,000 rpm for 1 min. Supernatants were discarded and cells were washed by sterile water for twice. Cells were resuspended in 20 mL minimal medium with initial OD of 0.05, pH 6.0, consisting of the following components: 20 g/L glucose, 14.4 g/L KH2PO4, 7.5 g/L (NH4)2SO4, 0.5 g/L MgSO4·7H2O, trace metal, vitamin solution, 40 mg/L histidine and 40 mg/L uracil [57], and incubated at 30 °C, 250 rpm. Cells were sampled for transcriptome analysis when OD600 reached 1.

After sampling, total RNA was extracted using the Yeast RNA Kit (Omega). The RNA sequencing was carried out in Novogene Co., Ltd. (Beijing, China). Illumina RNA-Seq data were aligned on the yeast genome using Bowtie2 [58]. Transcript abundance was estimated by method RSEM [59]. Differential expression analysis was processed by edgeR package in the R programming language [60]. Reporter analysis on GO terms and transcription factors was carried out via the Platform for Integrative Analysis of Omics (PIANO) R package [13]. GO slim mapping file was downloaded from SGD (http://sgd-archive.yeastgenome.org/) and gene-TF interaction pairs were obtained from YeasTMine (http://yeastmine.yeastgenome.org).

Construction of biosynthesis pathways

L-lactate dehydrogenase (LlLDH) was from Lactococcus lactis NZ9000. Acetolactate synthase (cytoILV2) was native S. cerevisiae gene but was truncated (2–90 aa) [8] to relocate it to the cytoplasm. Both LlLDH and cytoILV2 were inserted into plasmid pSP-GM2 between the restriction sites BamHI and NheI to construct plasmids used for production of lactate and 2,3-BD, respectively. Malonyl-CoA reductase (CaMCR), α-farnesene synthase (MdFS) and tyrosine ammonia lyase (FjTAL), from Chloroflexus aurantiacus [46], Malus domestica [61] and Flavobacterium johnsoniae [62], respectively, were codon optimized and placed under the control of TEF1 promoter, with their expression cassettes subsequently integrated into chromosomal site XII-2 to construct strains producing 3-HP, farnesene and p-coumaric acid. Similarly, geranylgeranyl pyrophosphate synthase (PaCrtE), phytoene synthase (PaCrtB) and phytoene desaturase (PaCrtI), all from Pantoea ananatis, were codon optimized, with their expression placed under the control of the promoters CDC19, CCW12 and TDH3, respectively. As before, the expression cassettes were then integrated into chromosomal site XII-2 to construct lycopene-producing strains. FFAs-producing strains were constructed by deleting FAA1, FAA4, POX1 and PAH1.

Expression formats were chosen according to previous study. As reported, 2,3-BD [16, 63,64,65] and lactate [20, 66,67,68] were widely produced by expressing genes in plasmids; meanwhile, p-coumaric acid [21, 29, 69,70,71], lycopene [44, 45, 72, 73], farnesene [3, 43, 74] and 3-HP [75] were widely produced by integrating genes into genome. Using the same expression format as reported will be of referential significance for demonstrating the biosynthetic capacity of chassis cell.

All the plasmids and expression cassettes were transformed into yeast by LiAC/ssDNA method [76]. Expression cassettes were integrated by CRISPR/Cas9 system. All strains used in this study are listed in Table 1. All primers, gRNA and deleting donors used in this study were summarized in Additional file 1: Tables S1 and S2.

Metabolite extraction and analysis

3-HP and lactate were measured at 65 °C by an HPLC system equipped with a refractive-index detector and a Bio-Rad HPX-87H column using 0.5 mM H2SO4 as mobile phase at a flow rate of 0.6 mL min−1. Esterification and analysis of FFAs were performed as previously described [78]. 2,3-BD was detected by the same methods as 3-HP, except for the use of 5 mM H2SO4 as the mobile phase and column temperature of 28 °C. Lycopene and farnesene were detected by HPLC equipped with an Innoval C18 column. The extracted and analyzed method was described previously [45]. p-Coumaric acid was detected by HPLC equipped with Discovery HS F5 150 mm × 2.1 mm column, as described in a previous study [62].

All data were presented as the mean of three biological replicates with error bars representing the standard deviations. P values were generated by performing t tests for determining statistical significance.

Fed-batch fermentation of free fatty acids in 5 L bioreactor

Saccharomyces cerevisiae was transferred from glycerol stock to 5 mL SD-URA medium and incubated at 30 °C and 250 rpm. Transfer the culture to 200 mL minimal medium with initial OD of 0.05. Once the strains reached the log-phase, they were transferred to a 5 L bioreactor containing 1.5 L batch medium, pH 6.0, consisting of 20 g/L glucose, 5 g/L (NH4)2SO4, 3 g/L KH2PO4, 0.5 g/L MgSO4·7H2O, 40 mg/L URA, 40 mg/L histidine, trace metal and vitamin solutions. Fed batch medium contained 600 g/L glucose, and 7 g/L (NH4)2SO4, 15 g/L KH2PO4, 2.5 g/L MgSO4·7H2O, 200 mg/L URA, 200 mg/L histidine, fivefolds of trace metal and vitamin solutions.

Availability of data and materials

The data sets generated during this study are included in this article and its additional files.

References

  1. Shen B, Zhou P, Jiao X, Yao Z, Ye L, Yu H. Fermentative production of vitamin E tocotrienols in Saccharomyces cerevisiae under cold-shock-triggered temperature control. Nat Commun. 2020;11(1):1–14.

    Article  Google Scholar 

  2. Avalos JL, Fink GR, Stephanopoulos G. Compartmentalization of metabolic pathways in yeast mitochondria improves the production of branched-chain alcohols. Nat Biotechnol. 2013;31(4):335–41.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  3. Meadows AL, Hawkins KM, Tsegaye Y, Antipov E, Kim Y, Raetz L, et al. Rewriting yeast central carbon metabolism for industrial isoprenoid production. Nature. 2016;537(7622):694–7.

    Article  CAS  PubMed  Google Scholar 

  4. Paddon CJ, Westfall PJ, Pitera DJ, Benjamin K, Fisher K, McPhee D, et al. High-level semi-synthetic production of the potent antimalarial artemisinin. Nature. 2013;496(7446):528–32.

    Article  CAS  PubMed  Google Scholar 

  5. 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(7):2402–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  6. 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(2):192–5.

    Article  CAS  PubMed  Google Scholar 

  7. Nielsen J. Synthetic biology for engineering acetyl coenzyme A metabolism in yeast. MBio. 2014;5(6):e02153-14.

    Article  PubMed  PubMed Central  Google Scholar 

  8. Lian J, Chao R, Zhao H. 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.

    Article  CAS  PubMed  Google Scholar 

  9. van Maris AJ, Geertman JM, Vermeulen A, Groothuizen MK, Winkler AA, Piper MD, et al. Directed evolution of pyruvate decarboxylase-negative Saccharomyces cerevisiae, yielding a C2-independent, glucose-tolerant, and pyruvate-hyperproducing yeast. Appl Environ Microbiol. 2004;70(1):159–66.

    Article  PubMed  PubMed Central  Google Scholar 

  10. Oud B, Flores CL, Gancedo C, Zhang X, Trueheart J, Daran JM, et al. An internal deletion in MTH1 enables growth on glucose of pyruvate-decarboxylase negative, non-fermentative Saccharomyces cerevisiae. Microb Cell Fact. 2012;11(131):1–10.

    Google Scholar 

  11. Lian J, Si T, Nair NU, Zhao H. Design and construction of acetyl-CoA overproducing Saccharomyces cerevisiae strains. Metab Eng. 2014;24:139–49.

    Article  CAS  PubMed  Google Scholar 

  12. Dai Z, Huang M, Chen Y, Siewers V, Nielsen J. Global rewiring of cellular metabolism renders Saccharomyces cerevisiae Crabtree negative. Nat Commun. 2018;9:1–8.

    Article  Google Scholar 

  13. Varemo L, Nielsen J, Nookaew I. Enriching the gene set analysis of genome-wide data by incorporating directionality of gene expression and combining statistical hypotheses and methods. Nucleic Acids Res. 2013;41(8):4378–91.

    Article  PubMed  PubMed Central  Google Scholar 

  14. Regenberg B, Grotkjaer T, Winther O, Fausboll A, Akesson M, Bro C, et al. Growth-rate regulated genes have profound impact on interpretation of transcriptome profiling in Saccharomyces cerevisiae. Genome Biol. 2006;7(11):R107.

    Article  PubMed  PubMed Central  Google Scholar 

  15. Malina C, Yu R, Bjorkeroth J, Kerkhoven EJ, Nielsen J. Adaptations in metabolism and protein translation give rise to the Crabtree effect in yeast. Proc Natl Acad Sci USA. 2021;118(51): e2112836118.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  16. Kim SJ, Seo SO, Jin YS, Seo JH. Production of 2,3-butanediol by engineered Saccharomyces cerevisiae. Bioresour Technol. 2013;146:274–81.

    Article  CAS  PubMed  Google Scholar 

  17. Ng C, Jung M-Y, Lee J, Oh M-K. Production of 2,3-butanediol in Saccharomyces cerevisiae by in silico aided metabolic engineering. Microb Cell Factories. 2012;11(1):68.

    Article  CAS  Google Scholar 

  18. Lodi T, Alberti A, Guiard B, Ferrero I. Regulation of the Saccharomyces cerevisiae DLD1 gene encoding the mitochondrial protein d-lactate ferricytochrome c oxidoreductase by HAP1 and HAP2/3/4/5. Mol Gen Genet. 1999;262(4):623–32.

    Article  CAS  PubMed  Google Scholar 

  19. Ramil E, Agrimonti C, Shechter E, Gervais M, Guiard B. Regulation of the CYB2 gene expression: transcriptional co-ordination by the Hap1p, Hap2/3/4/5p and Adr1p transcription factors. Mol Microbiol. 2000;37(5):1116–32.

    Article  CAS  PubMed  Google Scholar 

  20. Watcharawipas A, Sae-Tang K, Sansatchanon K, Sudying P, Boonchoo K, Tanapongpipat S, et al. Systematic engineering of Saccharomyces cerevisiae for d-lactic acid production with near theoretical yield. FEMS Yeast Res. 2021;21(4): foab024.

    Article  CAS  PubMed  Google Scholar 

  21. Borja GM, Rodriguez A, Campbell K, Borodina I, Chen Y, Nielsen J. Metabolic engineering and transcriptomic analysis of Saccharomyces cerevisiae producing p-coumaric acid from xylose. Microb Cell Fact. 2019;18(1):191.

    Article  PubMed  PubMed Central  Google Scholar 

  22. Mao J, Liu Q, Song X, Wang H, Feng H, Xu H, et al. Combinatorial analysis of enzymatic bottlenecks of l-tyrosine pathway by p-coumaric acid production in Saccharomyces cerevisiae. Biotechnol Lett. 2017;39(7):977–82.

    Article  CAS  PubMed  Google Scholar 

  23. Pyne ME, Narcross L, Melgar M, Kevvai K, Mookerjee S, Leite GB, et al. An engineered Aro1 protein degradation approach for increased cis, cis-muconic acid biosynthesis in Saccharomyces cerevisiae. Appl Environ Microbiol. 2018;84(17):e01095-e1118.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  24. Bisquert R, Planells-Carcel A, Valera-Garcia E, Guillamon JM, Muniz-Calvo S. Metabolic engineering of Saccharomyces cerevisiae for hydroxytyrosol overproduction directly from glucose. Microb Biotechnol. 2022;15(5):1499–510.

    Article  CAS  PubMed  Google Scholar 

  25. Luttik MA, Vuralhan Z, Suir E, Braus GH, Pronk JT, Daran JM. Alleviation of feedback inhibition in Saccharomyces cerevisiae aromatic amino acid biosynthesis: quantification of metabolic impact. Metab Eng. 2008;10(3–4):141–53.

    Article  CAS  PubMed  Google Scholar 

  26. Yin S, Lang T, Xiao X, Liu L, Sun B, Wang C. Significant enhancement of methionol production by co-expression of the aminotransferase gene ARO8 and the decarboxylase gene ARO10 in Saccharomyces cerevisiae. FEMS Microbiol Lett. 2015;362(5): fnu043.

    Article  PubMed  Google Scholar 

  27. Kim B, Cho BR, Hahn JS. Metabolic engineering of Saccharomyces cerevisiae for the production of 2-phenylethanol via Ehrlich pathway. Biotechnol Bioeng. 2014;111(1):115–24.

    Article  CAS  PubMed  Google Scholar 

  28. Romagnoli G, Luttik MA, Kotter P, Pronk JT, Daran JM. Substrate specificity of thiamine pyrophosphate-dependent 2-oxo-acid decarboxylases in Saccharomyces cerevisiae. Appl Environ Microbiol. 2012;78(21):7538–48.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  29. Rodriguez A, Chen Y, Khoomrung S, Ozdemir E, Borodina I, Nielsen J. Comparison of the metabolic response to over-production of p-coumaric acid in two yeast strains. Metab Eng. 2017;44:265–72.

    Article  CAS  PubMed  Google Scholar 

  30. Giovannucci E, Ascherio A, Rimm EB, Stampfer MJ, Colditz GA, Willett WC. Intake of carotenoids and retino in relation to risk of prostate cancer. J Natl Cancer Inst. 1995;87(23):1767–76.

    Article  CAS  PubMed  Google Scholar 

  31. Sies H, Stahl W. Lycopene: antioxidant and biological effects and its bioavailability in the human. Proc Soc Exp Biol Med. 1998;218(2):121–4.

    Article  CAS  PubMed  Google Scholar 

  32. Hiser L, Basson ME, Rine J. ERG10 from Saccharomyces cerevisiae encodes acetoacetyl-CoA thiolase. J Biol Chem. 1994;269(50):31383–9.

    Article  CAS  PubMed  Google Scholar 

  33. Basson ME, Thorsness M, Rine J. Saccharomyces cerevisiae contains two functional genes encoding 3-hydroxy-3-methylglutaryl-coenzyme A reductase. Proc Nati Acad Sci USA. 1988;83:5563–7.

    Article  Google Scholar 

  34. Anderson MS, Muehlbacher M, Street I, Proffitt J, Poulter C. Isopentenyl diphosphate: dimethylallyl diphosphate isomerase: an improved purification of the enzyme and isolation of the gene from Saccharomyces cerevisiae. J Bio Chem. 1989;264(32):19169–75.

    Article  CAS  Google Scholar 

  35. Bergès T, Guyonnet D, Karst F. The Saccharomyces cerevisiae mevalonate diphosphate decarboxylase is essential for viability, and a single Leu-to-Pro mutation in a conserved sequence leads to thermosensitivity. J Bacteriol. 1997;179(15):4664–70.

    Article  PubMed  PubMed Central  Google Scholar 

  36. Anderson MS, Yarger JG, Burck CL, Poulter CD. Farnesyl diphosphate synthetase. Molecular cloning, sequence, and expression of an essential gene from Saccharomyces cerevisiae. J Biol Chem. 1989;264(32):19176–84.

    Article  CAS  PubMed  Google Scholar 

  37. Jiang Y, Proteau P, Poulter D, Ferro-Novick S. BTS1 encodes a geranylgeranyl diphosphate synthase in Saccharomyces cerevisiae. J Bio Chem. 1995;270(37):21793–9.

    Article  CAS  Google Scholar 

  38. Lv X, Xie W, Lu W, Guo F, Gu J, Yu H, et al. Enhanced isoprene biosynthesis in Saccharomyces cerevisiae by engineering of the native acetyl-CoA and mevalonic acid pathways with a push–pull–restrain strategy. J Biotechnol. 2014;186:128–36.

    Article  CAS  PubMed  Google Scholar 

  39. Tokuhiro K, Muramatsu M, Ohto C, Kawaguchi T, Obata S, Muramoto N, et al. Overproduction of geranylgeraniol by metabolically engineered Saccharomyces cerevisiae. Appl Environ Microbiol. 2009;75(17):5536–43.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  40. Jiang G-Z, Yao M-D, Wang Y, Zhou L, Song T-Q, Liu H, et al. Manipulation of GES and ERG20 for geraniol overproduction in Saccharomyces cerevisiae. Metab Eng. 2017;41:57–66.

    Article  CAS  PubMed  Google Scholar 

  41. Yao Z, Zhou P, Su B, Su S, Ye L, Yu H. Enhanced isoprene production by reconstruction of metabolic balance between strengthened precursor supply and improved isoprene synthase in Saccharomyces cerevisiae. ACS Synth Biol. 2018;7(9):2308–16.

    Article  CAS  PubMed  Google Scholar 

  42. Mantzouridou F, Tsimidou MZ. Observations on squalene accumulation in Saccharomyces cerevisiae due to the manipulation of HMG2 and ERG6. FEMS Yeast Res. 2010;10(6):699–707.

    Article  CAS  PubMed  Google Scholar 

  43. Wang J, Jiang W, Liang C, Zhu L, Li Y, Mo Q, et al. Overproduction of alpha-farnesene in Saccharomyces cerevisiae by farnesene synthase screening and metabolic engineering. J Agric Food Chem. 2021;69(10):3103–13.

    Article  CAS  PubMed  Google Scholar 

  44. Chen Y, Xiao W, Wang Y, Liu H, Li X, Yuan Y. Lycopene overproduction in Saccharomyces cerevisiae through combining pathway engineering with host engineering. Microb Cell Fact. 2016;15(1):113.

    Article  PubMed  PubMed Central  Google Scholar 

  45. Xie W, Lv X, Ye L, Zhou P, Yu H. Construction of lycopene-overproducing Saccharomyces cerevisiae by combining directed evolution and metabolic engineering. Metab Eng. 2015;30:69–78.

    Article  CAS  PubMed  Google Scholar 

  46. Chen Y, Bao J, Kim IK, Siewers V, Nielsen J. Coupled incremental precursor and co-factor supply improves 3-hydroxypropionic acid production in Saccharomyces cerevisiae. Metab Eng. 2014;22:104–9.

    Article  PubMed  Google Scholar 

  47. Ferreira R, Teixeira PG, Siewers V, Nielsen J. Redirection of lipid flux toward phospholipids in yeast increases fatty acid turnover and secretion. Proc Natl Acad Sci USA. 2018;115(6):1262–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  48. Singh SK, Ahmed SU, Pandey A. Metabolic engineering approaches for lactic acid production. Process Biochem. 2006;41(5):991–1000.

    Article  CAS  Google Scholar 

  49. Yang Z, Zhang Z. Recent advances on production of 2, 3-butanediol using engineered microbes. Biotechnol Adv. 2019;37(4):569–78.

    Article  CAS  PubMed  Google Scholar 

  50. Hügler M, Menendez C, Schägger H, Fuchs G. Malonyl-coenzyme A reductase from Chloroflexus aurantiacus, a key enzyme of the 3-hydroxypropionate cycle for autotrophic CO2 fixation. J Bacteriol. 2002;184(9):2404–10.

    Article  PubMed  PubMed Central  Google Scholar 

  51. Partow S, Siewers V, Daviet L, Schalk M, Nielsen J. Reconstruction and evaluation of the synthetic bacterial MEP pathway in Saccharomyces cerevisiae. PLoS ONE. 2012;7(12): e52498.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  52. Yu T, Zhou YJ, Huang M, Liu Q, Pereira R, David F, et al. Reprogramming yeast metabolism from alcoholic fermentation to lipogenesis. Cell. 2018;174(6):1549–58.

    Article  CAS  PubMed  Google Scholar 

  53. Garay-Arroyo A, Covarrubias AA, Clark I, Nino I, Gosset G, Martinez A. Response to different environmental stress conditions of industrial and laboratory Saccharomyces cerevisiae strains. Appl Microbiol Biotechnol. 2004;63(6):734–41.

    Article  CAS  PubMed  Google Scholar 

  54. Ledesma-Amaro R, Dulermo R, Niehus X, Nicaud JM. Combining metabolic engineering and process optimization to improve production and secretion of fatty acids. Metab Eng. 2016;38:38–46.

    Article  CAS  PubMed  Google Scholar 

  55. Fang L, Fan J, Luo S, Chen Y, Wang C, Cao Y, et al. Genome-scale target identification in Escherichia coli for high-titer production of free fatty acids. Nat Commun. 2021;12(1):4976.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  56. Sun T, Miao L, Li Q, Dai G, Lu F, Liu T, et al. Production of lycopene by metabolically-engineered Escherichia coli. Biotechnol Lett. 2014;36(7):1515–22.

    Article  CAS  PubMed  Google Scholar 

  57. Verduyn C, Postma E, Scheffers WA, Van Dijken JP. Effect of benzoic acid on metabolic fluxes in yeasts: a continuous-culture study on the regulation of respiration and alcoholic fermentation. Yeast. 1992;8:501–17.

    Article  CAS  PubMed  Google Scholar 

  58. Langmead B, Salzberg SL. Fast gapped-read alignment with Bowtie 2. Nat Methods. 2012;9(4):357–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  59. Li B, Dewey CN. RSEM: accurate transcript quantification from RNA-Seq data with or without a reference genome. BMC Bioinform. 2011;12(1):1–16.

    Article  Google Scholar 

  60. Robinson MD, McCarthy DJ, Smyth GK. edgeR: a Bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics. 2010;26(1):139–40.

    Article  CAS  PubMed  Google Scholar 

  61. Tippmann S, Scalcinati G, Siewers V, Nielsen J. Production of farnesene and santalene by Saccharomyces cerevisiae using fed-batch cultivations with RQ-controlled feed. Biotechnol Bioeng. 2016;113(1):72–81.

    Article  CAS  PubMed  Google Scholar 

  62. Liu Q, Yu T, Li X, Chen Y, Campbell K, Nielsen J, et al. Rewiring carbon metabolism in yeast for high level production of aromatic chemicals. Nat Commun. 2019;10(1):4976.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  63. Kim S, Hahn JS. Synthetic scaffold based on a cohesin-dockerin interaction for improved production of 2,3-butanediol in Saccharomyces cerevisiae. J Biotechnol. 2014;192(Pt A):192–6.

    Article  CAS  PubMed  Google Scholar 

  64. Ng C, Jung M-Y, Lee J, Oh M-K. Production of 2,3-butanediol in Saccharomyces cerevisiae by in silico aided metabolic engineering. Microb Cell Fact. 2012;11(1):68.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  65. Kim S, Hahn J-S. Efficient production of 2,3-butanediol in Saccharomyces cerevisiae by eliminating ethanol and glycerol production and redox rebalancing. Metab Eng. 2015;31:94–101.

    Article  CAS  PubMed  Google Scholar 

  66. Tokuhiro K, Ishida N, Nagamori E, Saitoh S, Onishi T, Kondo A, et al. 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(5):883–90.

    Article  CAS  PubMed  Google Scholar 

  67. Skory CD. Lactic acid production by Saccharomyces cerevisiae expressing a Rhizopus oryzae lactate dehydrogenase gene. J Ind Microbiol Biotechnol. 2003;30(1):22–7.

    Article  CAS  PubMed  Google Scholar 

  68. Ishida N, Saitoh S, Tokuhiro K, Nagamori E, Matsuyama T, Kitamoto K, et al. Efficient production of l-lactic acid by metabolically engineered Saccharomyces cerevisiae with a genome-integrated l-lactate dehydrogenase gene. Appl Environ Microbiol. 2005;71(4):1964–70.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  69. Combes J, Imatoukene N, Couvreur J, Godon B, Fojcik C, Allais F, et al. An optimized semi-defined medium for p-coumaric acid production in extractive fermentation. Process Biochem. 2022;122:357–62.

    Article  CAS  Google Scholar 

  70. Combes J, Imatoukene N, Couvreur J, Godon B, Brunissen F, Fojcik C, et al. Intensification of p-coumaric acid heterologous production using extractive biphasic fermentation. Bioresour Technol. 2021;337: 125436.

    Article  CAS  PubMed  Google Scholar 

  71. Qi H, Li Y, Cai M, He J, Liu J, Song X, et al. High-copy genome integration and stable production of p-coumaric acid via a POT1-mediated strategy in Saccharomyces cerevisiae. J Appl Microbiol. 2022;133(2):707–19.

    Article  CAS  PubMed  Google Scholar 

  72. Hong J, Park SH, Kim S, Kim SW, Hahn JS. Efficient production of lycopene in Saccharomyces cerevisiae by enzyme engineering and increasing membrane flexibility and NAPDH production. Appl Microbiol Biotechnol. 2019;103(1):211–23.

    Article  CAS  PubMed  Google Scholar 

  73. Ma T, Shi B, Ye Z, Li X, Liu M, Chen Y, et al. Lipid engineering combined with systematic metabolic engineering of Saccharomyces cerevisiae for high-yield production of lycopene. Metab Eng. 2019;52:134–42.

    Article  CAS  PubMed  Google Scholar 

  74. Sandoval CM, Ayson M, Moss N, Lieu B, Jackson P, Gaucher SP, et al. Use of pantothenate as a metabolic switch increases the genetic stability of farnesene producing Saccharomyces cerevisiae. Metab Eng. 2014;25:215–26.

    Article  CAS  PubMed  Google Scholar 

  75. Kildegaard KR, Jensen NB, Schneider K, Czarnotta E, Ozdemir E, Klein T, et al. Engineering and systems-level analysis of Saccharomyces cerevisiae for production of 3-hydroxypropionic acid via malonyl-CoA reductase-dependent pathway. Microb Cell Fact. 2016;15:53.

    Article  PubMed  PubMed Central  Google Scholar 

  76. Gietz RD, Schiestl RH. High-efficiency yeast transformation using the LiAc/SS carrier DNA/PEG method. Nat Protoc. 2007;2(1):31–4.

    Article  CAS  PubMed  Google Scholar 

  77. Zhang Y, Liu G, Engqvist MKM, Krivoruchko A, Hallström BM, Chen Y, et al. Adaptive mutations in sugar metabolism restore growth on glucose in a pyruvate decarboxylase negative yeast strain. Microb Cell Fact. 2015;14(116):1–11.

    Google Scholar 

  78. Khoomrung S, Chumnanpuen P, Jansa-ard S, Nookaew I, Nielsen J. Fast and accurate preparation fatty acid methyl esters by microwave-assisted derivatization in the yeast Saccharomyces cerevisiae. Appl Microbiol Biotechnol. 2012;94(6):1637–46.

    Article  CAS  PubMed  Google Scholar 

Download references

Acknowledgements

We thank Dr. Quanli Liu, Dr. Xiaowei Li, Dr. Qi for their help with data collection.

Funding

This work was supported by the National Natural Science Foundation of China (32071423, 32161133019), Hundreds of Talents Program of the Chinese Academy of Sciences (Y0J51009), Tianjin Synthetic Biotechnology Innovation Capacity Improvement Project (TSBICIP-CXRC-002) and the Novo Nordisk Foundation (NNF10CC1016517).

Author information

Authors and Affiliations

  1. Tianjin Institute of Industrial Biotechnology, Chinese Academy of Sciences, Tianjin, 300308, China

    Zhen Yao, Yufeng Guo, Qinhong Wang & Zongjie Dai

  2. National Center of Technology Innovation for Synthetic Biology, Tianjin, 300308, China

    Zhen Yao, Yufeng Guo, Qinhong Wang & Zongjie Dai

  3. Laboratory of Evolutionary and Functional Genomics, School of Life Sciences, Chongqing University, Chongqing, 401331, China

    Huan Wang

  4. Department of Biology and Biological Engineering, Chalmers University of Technology, 412 96, Gothenburg, Sweden

    Yun Chen & Jens Nielsen

  5. Beijing Advanced Innovation Center for Soft Matter Science and Engineering, College of Life Science and Technology, Beijing University of Chemical Technology, Beijing, 100029, China

    Jens Nielsen

Authors
  1. Zhen Yao
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Yufeng Guo
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Huan Wang
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Yun Chen
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Qinhong Wang
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Jens Nielsen
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Zongjie Dai
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

ZY and ZD designed the research; ZY performed the experiments; ZY, YG, HW, YC and ZD analyzed the data; ZY and ZD wrote and revised the manuscript; QW, JN and ZD supervised the project. All authors read and approved the final manuscript.

Corresponding authors

Correspondence to Jens Nielsen or Zongjie Dai.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare no competing interests.

Additional information

Publisher's Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary Information

Additional file 1: Figure S1.

Reporter transcription factors (TFs) analysis of strain sZJD-28 compared with CEN.PK 113-11C. Figure S2. Fold changes of transcriptional levels of ILV2, HXT1, HXT3, CYB2, DLD1, ACC1, FAS1 and FAS2 in sZJD-28 relative to CEN.PK113-11C. Figure S3. Production of lactate by Crabtree positive 11C-LA and negative 28-LA. Table S1. Primers used in this study. Table S2. gRNA and deleting donors used in this study.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Yao, Z., Guo, Y., Wang, H. et al. A highly efficient transcriptome-based biosynthesis of non-ethanol chemicals in Crabtree negative Saccharomyces cerevisiae. Biotechnol Biofuels 16, 37 (2023). https://doi.org/10.1186/s13068-023-02276-5

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s13068-023-02276-5

Keywords

Biotechnology for Biofuels and Bioproducts

ISSN: 2731-3654

Contact us