- Open Access
Metabolic engineering of Zymomonas mobilis for anaerobic isobutanol production
Biotechnology for Biofuels volume 13, Article number: 15 (2020)
Biofuels and value-added biochemicals derived from renewable biomass via biochemical conversion have attracted considerable attention to meet global sustainable energy and environmental goals. Isobutanol is a four-carbon alcohol with many advantages that make it attractive as a fossil-fuel alternative. Zymomonas mobilis is a highly efficient, anaerobic, ethanologenic bacterium making it a promising industrial platform for use in a biorefinery.
In this study, the effect of isobutanol on Z. mobilis was investigated, and various isobutanol-producing recombinant strains were constructed. The results showed that the Z. mobilis parental strain was able to grow in the presence of isobutanol below 12 g/L while concentrations greater than 16 g/L inhibited cell growth. Integration of the heterologous gene encoding 2-ketoisovalerate decarboxylase such as kdcA from Lactococcus lactis is required for isobutanol production in Z. mobilis. Moreover, isobutanol production increased from nearly zero to 100–150 mg/L in recombinant strains containing the kdcA gene driven by the tetracycline-inducible promoter Ptet. In addition, we determined that overexpression of a heterologous als gene and two native genes (ilvC and ilvD) involved in valine metabolism in a recombinant Z. mobilis strain expressing kdcA can divert pyruvate from ethanol production to isobutanol biosynthesis. This engineering improved isobutanol production to above 1 g/L. Finally, recombinant strains containing both a synthetic operon, als-ilvC-ilvD, driven by Ptet and the kdcA gene driven by the constitutive strong promoter, Pgap, were determined to greatly enhance isobutanol production with a maximum titer about 4.0 g/L. Finally, isobutanol production was negatively affected by aeration with more isobutanol being produced in more poorly aerated flasks.
This study demonstrated that overexpression of kdcA in combination with a synthetic heterologous operon, als-ilvC-ilvD, is crucial for diverting pyruvate from ethanol production for enhanced isobutanol biosynthesis. Moreover, this study also provides a strategy for harnessing the valine metabolic pathway for future production of other pyruvate-derived biochemicals in Z. mobilis.
Current global environment concerns provide motivation for the development of renewable and sustainable biofuels production technologies [1, 2]. In recent years, many microorganisms have been developed to produce eco-friendly, renewable biofuels using metabolic engineering and synthetic biology [3, 4]. Although bioethanol is the most studied bio-based fuel and lignocellulosic ethanol production has been successfully established in several countries, the intrinsic properties of bioethanol, such as high hygroscopicity, high vapor pressure, and low energy density limit its application in specific cases, such as jet fuel [5,6,7]. In contrast, higher alcohols, such as isobutanol, possess several advantages. These include higher energy density, low hygroscopicity, low vapor pressure, and high-octane number. Isobutanol can also serve as a precursor for the production of isobutene, making it a promising alternative for current fossil fuels [6, 8, 9]. In fact, Gevo Inc. has announced that it will develop and deploy isobutanol as a jet-fuel additive from renewable feedstocks (http://ir.gevo.com).
Zymomonas mobilis is a Gram-negative, natural bacterial ethanologen with many desirable industrial characteristics, such as a high specific rate of glucose uptake, low biomass production, low aeration cost due to anaerobic fermentation, and a high ethanol tolerance up to 16% (v/v) [2, 10,11,12]. Z. mobilis has been engineered to broaden its range of fermentable substrates, which now include the pentoses (xylose and arabinose) , and to expand its range of fermentation products to include 2,3-butanediol and lactic acid [1, 2, 4, 10, 14,15,16]. In addition, the genome sequence, functional re-annotation, and substantial systems biology studies and metabolic models of Z. mobilis have been reported [12, 15, 17,18,19,20,21,22,23,24]. Recent development of genome editing such as exogenous and native CRISPR-cas toolkits as well as methods for biological part identification and characterization [25,26,27,28,29,30,31] will facilitate heterologous pathway engineering and unravel the underlying mechanisms for balanced production and robustness  in Z. mobilis.
The isobutanol biosynthesis pathway involves five enzymes. First, acetolactate synthase (Als, EC126.96.36.199) catalyzes the condensation of two pyruvates to generate acetolactate, which is then reduced to 2,3-dihydroxyisovalerate by ketol-acid reductoisomerase (IlvC, EC188.8.131.52). This intermediate is subsequently converted to 2-ketoisovalerate by dihydroxy-acid dehydratase (IlvD, EC184.108.40.206), and further converted to isobutyraldehyde and alcohols (e.g., isobutanol) subsequently by 2-ketoisovalerate decarboxylase (Kdc) and alcohol dehydrogenase (Adh). Als usually contains a large subunit with catalytic function and a small (regulatory) subunit involved in substrate specificity, valine sensitivity and cofactor affinity, respectively. The first three enzymes are shared with the l-valine biosynthesis pathway, which exists in most microorganisms. Adh enzymes are also widespread in nearly all microorganisms. However, the essential enzyme, Kdc, for isobutanol production is absent in most bacteria including Z. mobilis. But some species of yeasts, fungi, and plants possess this enzyme , which can be introduced into microorganisms for heterologous isobutanol production.
The isobutanol biosynthesis pathway has been engineered into various microorganisms, such as Escherichia coli , Saccharomyces cerevisiae [7, 34], Pichia pastoris , Bacillus subtilis , Corynebacterium glutamicum [8, 37], Geobacillus thermoglucosidasius , and Synechocystis PCC 6803 [39,40,41]. For example, Atsumi et al. engineered E. coli to produce isobutanol up to 22 g/L in shake flasks [33, 42], which was further increased to 50 g/L in bioreactors during batch cultures with in situ product removal by gas stripping . Recently, Ghosh and co-workers optimized their constructs based on models to predict the impacts of enzyme synthesis cost on cellular growth rates and obtained a recombinant strain with an isobutanol productivity of 3 g/h/g DCW (dry ell weight) . Li and co-workers found that B. subtilis was a feasible host because it had a higher isobutanol tolerance than E. coli and C. glutamicum and produced up to 2.62 g/L isobutanol during fed-batch fermentation .
Atsumi and coworkers also introduced the isobutanol biosynthesis pathway genes from several species into the cyanobacterium Synechococcus elongatus PCC7942, confirming that the microorganism was able to produce an isobutanol titer of 450 mg/L directly from carbon dioxide . Isobutanol production from Synechocystis PCC 6803 was also investigated and shown to achieve a cumulative titer of 911 mg/L following implementation of new metabolic engineering strategies [39, 40, 46].
As for eukaryotes, Chen and co-workers examined the feasibility of exploring S. cerevisiae as a potential platform microorganism for higher alcohols production. By overexpressing the ilv2, ilv3, and ilv5 genes involved in valine metabolism, the authors were able to achieve an isobutanol yield of 3.86 mg/g glucose under aerobic conditions . This isobutanol yield was further elevated to 6.6 mg/g glucose by overexpressing kivd, as well as Adh6 and ilv2 to enhance the endogenous enzyme activities necessary for isobutanol production. pdc1 was also deleted to temper ethanol flux via pyruvate .
Despite of significant progress achieved on isobutanol production in various microorganisms, most require aerobic fermentation conditions, a costly input for industrial production. In addition, current efforts on improving isobutanol production in these microorganisms have been focused on increasing the pyruvate pool, eliminating by-product formation, and maintaining redox balance [44, 47,48,49,50,51]. For example, the Entner–Doudoroff (ED) pathway was applied into E. coli, and the ED pathway-dependent isobutanol-producing E. coli strain was further optimized to produce 15.0 g/L isobutanol after byproduct biosynthesis genes were inactivated . Z. mobilis can be a suitable host to address these issues since it has the characteristics of a unique anaerobic ED pathway, a truncated tricarboxylic acid cycle (TCA), and simple metabolism resulting in abundant pyruvate biosynthesis with redox balancing that limits by-product formation. In this study, a heterologous isobutanol production pathway was engineered into a facultative anaerobic bacterium, Z. mobilis, for anaerobic isobutanol production, which will not only generate recombinant strains for anaerobic isobutanol production, but also provide strategies to divert pyruvate from the prevailing ethanol biosynthesis to the potential production of other pyruvate-derived biochemicals.
Results and discussion
Investigation of isobutanol toxicity to Z. mobilis
In order to produce potentially toxic biochemicals like isobutanol with high titer, yield, and productivity, the host microorganism must have the capability to tolerate the product at increased concentrations. Therefore, isobutanol toxicity to Z. mobilis was investigated. As shown in Fig. 1, Z. mobilis cannot grow in medium with 20 g/L isobutanol supplementation and had a lag phase of more than 60 h before showing growth in medium containing 16 g/L isobutanol. Although Z. mobilis can grow with the supplementation of isobutanol at 12 g/L or lower, both growth rates and final OD600nm values were reduced correspondingly with the increase of supplemented isobutanol (Fig. 1). For example, compared to growth without isobutanol, the final OD600nm value with the presence of 12 g/L isobutanol decreased only slightly from 1.4 to 1.2 (Fig. 1a). However, under these conditions, the growth rate dropped by nearly half from 0.50 ± 0.00 to 0.275 ± 0.019 (Fig. 1b). The reduction in growth rate and the corresponding increase in isobutanol concentration were correlated (R-squared value of 0.96; y = − 0.0196x + 0.5179) (Fig. 1b).
Z. mobilis can tolerate ethanol up to 16% (v/v) . In our previous study, we characterized the toxicity of 2,3-butanediol on Z. mobilis and found that 2,3-butanediol was less toxic than ethanol and the supplementation of 100 g/L 2,3-butanediol only reduced growth rate by 20% . These results indicate that although isobutanol is more toxic than ethanol and 2,3-butanediol to Z. mobilis, a titer up to 12 g/L could be achieved without completely preventing cells from growing, an outcome which can potentially be optimized for isobutanol production through tolerance engineering. Gas stripping during fermentation could also be applied to remove the isobutanol in situ to increase the titer, yield, and productivity. Ultimately, more robust strains could be developed using mutagenesis and adaptive laboratory evolution (ALE).
Selection of genes for heterologous isobutanol production in Z. mobilis
Based on gene homology search results, Z. mobilis possesses four genes ZMO01139, ZMO1140, ZMO1141, and ZMO1792 encoding the enzymes Als, IlvC, and IlvD, respectively. ZMO01139 and ZMO1140 encode the large and small (regulatory) subunits of Als, respectively. These enzymes are the first three enzymes in the production of l-valine from pyruvate (Fig. 2). In addition, several alcohol dehydrogenases were also identified in Z. mobilis including a Zn-dependent alcohol dehydrogenase AdhA (ZMO1236); iron-containing alcohol dehydrogenases AdhB (ZMO1593) and ZMO1771; a Zn-dependent alcohol dehydrogenase class III AdhC (ZMO1722); and a plasmid-borne alcohol dehydrogenase-like protein (pZYM33_021).
Our previous study demonstrated that one of these five alcohol dehydrogenases contributes to 2,3-butanediol production , which may also be functional for the conversion of isobutyraldehyde to isobutanol although further study is needed to determine the roles of these Adh enzymes in the biosynthesis of different alcohols. The only enzyme required for isobutanol biosynthesis that was not identified in Z. mobilis is kdcA. The kdcA gene from Lactococcus lactis was used in previous studies for heterologous isobutanol production, which was selected and the codon-optimized kdcA gene was synthesized by GenScript (Nanjing, China) for subsequent study.
Introduction of kdcA into Z. mobilis for isobutanol production
The codon-optimized kdcA gene from L. lactis was cloned into the shuttle vector pEZ15Asp  generating the plasmid pEZ-KT, in which kdcA is driven by the tetracycline-inducible promoter Ptet. pEZ-KT was then introduced into Z. mobilis ZM4 to generate the recombinant strain ZM4-KT, and then confirmed by Sanger sequencing.
The impact of kdcA expression under the control of the Ptet promoter on isobutanol production was then investigated with different concentrations of tetracycline as an inducer ranging from 0 to 2 μg/mL. Isobutanol production was significantly improved with the increase of tetracycline concentrations (Fig. 3). When glucose was completely consumed (i.e., within 24 h of post-inoculation), the isobutanol titer was 89.33 ± 5.51 mg/L and 152.33 ± 13.05 mg/L with the induction of 1 and 2 μg/mL tetracycline, respectively. No isobutanol was detected without tetracycline induction (Fig. 3).
Although there were no significant differences in final ethanol titers (around 20 g/L) when induced by different concentrations of tetracycline, glucose consumption and ethanol production rates decreased with the increase of tetracycline concentrations (Fig. 3). Our previous study indicated that tetracycline negatively affected cellular growth of Z. mobilis above 2 μg/mL. However, tetracycline almost had no impact at concentrations below 1 μg/mL . Considering the titers of isobutanol were around 40–150 mg/L level, the decreased glucose utilization and ethanol production rates may be due to the impact of tetracycline on cellular function at high concentrations (i.e., 2 μg/mL). Tetracycline concentrations of 0, 0.2, and 1 μg/mL were therefore selected for subsequent experiments.
Construction of stable heterologous isobutanol production strains
Zymomonas mobilis ZM4 contains a 2.06 Mb genome with four native plasmids (pZM32 (32,791 bp), pZM33 (33,006 bp), pZM36 (36,494 bp), and pZM39 (39,266 bp) . ZMO0038 is a putative sigma 54 modulation protein and the deletion of ZMO0038 does not affect the growth of Z. mobilis . To construct a stable isobutanol production strain, the codon-optimized kdcA gene driven by Ptet was integrated into the genome at either the chromosomal locus of ZMO0038 or the native plasmid locus pZM36-005, resulting in the recombinant strains of ZMQ1 and ZMQ2, respectively (Fig. 4a). Tetracycline concentrations of 0, 0.2, and 1 μg/mL were used to induce the expression of kdcA for isobutanol production. ZMQ1 reached a maximum isobutanol titer of 104.33 ± 3.51 mg/L, which was 1.4 times higher than ZMQ2 with a titer of 74.67 ± 0.58 mg/L with 1 μg/mL tetracycline induction 24-h post-inoculation (Fig. 4b). Since the expression of the kdcA gene in the ZM4 genome at the ZMO0038 locus was better than in the native plasmid pZM36, ZMQ1 was selected for further experiments.
In addition, although the titer of isobutanol increased corresponding to the higher tetracycline concentrations, the final ethanol titer was nearly the same between ZMQ1 and ZMQ2 with both reaching approximately 20 g/L. These results indicated that the kdcA gene alone cannot effectively compete with ethanol production and another strategy is needed to divert carbon flux from ethanol production to isobutanol biosynthesis.
Overexpression of heterologous als and ilvC-ilvD to increase isobutanol production
Our previous work indicated that the addition of a heterologous Als is crucial to divert carbon flux from ethanol production to 2,3-butanediol biosynthesis . To enhance isobutanol production, a similar strategy was employed. Four als genes from different bacteria (ZmAls from Z. mobilis, EcAls from E. cloacae, BlAls from Bacillus licheniformis, and BsAls from B. subtilis) as well as ilvC and ilvD from Z. mobilis were selected and six plasmids were constructed (Fig. 5a). Since the als gene is driven by a strong promoter, Pgap, and may cause increased cellular metabolic burden consistent with our previous observations , an inducible promoter Ptet was utilized to control the expression of the synthetic operon containing the als, ilvC, and ilvD genes (Fig. 5a). We then examined the impacts on Z. mobilis isobutanol production by inducing Als alone, both IlvC and IlvD, and combinations of Als from four other bacteria. The IlvC and IlvD constructs contain a strong bacterial ribosomal binding site (RBS) (BBa_B0034) (Fig. 5b) are detailed below .
Isobutanol production in the recombinant strain, ZMQ1-B, containing the als gene from B. subtilis decreased to 75.33 ± 0.58 mg/L compared to 104.33 ± 3.51 mg/L in the host strain ZMQ1. Isobutanol production in the recombinant strains ZMQ1-A0 and ZMQ1-A1 containing plasmids pEZ-A0 and pEZ-A1 to overexpress ilvC and ilvD or all three genes ZmAls, ilvC, and ilvD also decreased to 38.33 ± 1.15 mg/L and 26.67 ± 2.08 mg/L, respectively, under the induction of 1 μg/mL tetracycline (Fig. 5b). These results suggest that the overexpression of only BsAls or ilvC and ilvD, or all three native genes ZmAls, ilvC, and ilvD, were not able to increase isobutanol production.
However, the overexpression of a heterologous operon containing an als gene (EcAls, BlAls, or BsAls) with both ilvC and ilvD in ZMQ1-A2, ZMQ1-A3, and ZMQ1-A4 increased isobutanol production to 0.82 ± 0.09 g/L, 1.05 ± 0.12 g/L, and 1.23 ± 0.05 g/L with the induction of 1 μg/mL tetracycline (Fig. 5b), which was about 8, 12, and 12.6 times of the isobutanol production in ZMQ1, respectively. Correlated with the increase of isobutanol production in ZMQ1-A2, ZMQ1-A3, and ZMQ1-A4, ethanol production decreased from 21.44 ± 0.11 g/L in ZMQ1 to 18.86 ± 0.96, 17.74 ± 0.89, and 17.75 ± 0.87 g/L in these recombinant strains, respectively (Fig. 5b). Ethanol production in the recombinant strains ZMQ1-A2, ZMQ1-A3, and ZMQ1-A4 without tetracycline induction was comparable to ZMQ1, with a titer of 20.67 ± 0.93, 19.21 ± 0.75, 20.03 ± 0.89, respectively. These results indicate that in Z. mobilis, a non-native als gene coupled with over-expression of the native ilvC-ilvD genes are necessary to divert carbon flux from ethanol production or native valine biosynthesis to isobutanol production.
Replacement of the inducible Ptet promoter driving kdcA with constitutive strong promoters to increase isobutanol production
The Ptet promoter was used in this study to evaluate the effects of overexpression of either the kdcA gene or the synthetic operon of als-ilvC-ilvD on isobutanol production. Our results demonstrated that by increasing the concentrations of the tetracycline inducer, isobutanol titers could also be increased (Figs. 3, 4, 5).
Our previous study on constructing the 2,3-butanediol production strains demonstrated that the expression of a synthetic operon aldC-bdh under the control of the constitutive strong promoter Pgap is crucial for high 2,3-BDO production, and the combination of Ptet driving the heterologous als gene with the Pgap driving aldC-bdh gave the maximum 2,3-BDO production with a titer of 13.3 ± 0.7 g/L . We therefore explored the possibility of increasing isobutanol production by replacing the Ptet promoter driving the kdcA gene with a strong promoter of Peno or Pgap while keeping Ptet to drive the expression of the als-ilvC-ilvD operon.
First, we replaced the Ptet promoter in ZMQ1 and ZMQ2 with the strong promoter Pgap and generated the new recombinant strains ZMQ3 (integration at the ZMO0038 chromosomal locus) and ZMQ4 (integration at the pZM36-005 native plasmid locus), respectively. In addition, the Ptet promoter was also replaced with another constitutive strong promoter, Peno, with integration at the ZMO0038 chromosomal locus to generate ZMQ 5 (Fig. 6a). The titers of isobutanol production in ZMQ3, ZMQ4, and ZMQ5 were 144.33 ± 7.23, 147.33 ± 1.15, and 120.00 ± 3.00 mg/L under the induction of 1 μg/mL tetracycline 12 h post-inoculation, respectively (Fig. 6b). The titers and productivities of ZMQ3, ZMQ4, and ZMQ5 were all significantly higher than those of ZMQ1 and ZMQ2, which were 104.33 ± 3.51 and 74.67 ± 0.58 mg/L after 24 h inoculation, respectively. Because isobutanol production in ZMQ3 and ZMQ4 were comparable to each other, but higher than that in ZMQ5, ZMQ3 with the kdcA gene driven by the constitutive strong promoter, Pgap, inserted into the ZMO0038 locus was selected for subsequent experiments.
Three plasmids (pEZ-A2, pEZ-A3, and pEZ-A4) with Ptet driving the expression of the synthetic operon, als-ilvC-ilvD (Fig. 5a), were then transformed into the recombinant ZMQ3 separately to generate the recombinant strains ZMQ3-A2, ZMQ3-A3, and ZMQ3-A4, respectively. Isobutanol production in these three recombinants was significantly higher than the parental strain ZMQ3 with the maximum isobutanol production in ZMQ3-A4 reaching 4.01 ± 0.06 g/L. The overexpression of the heterologous BsAls gene from B. subtilis was the most effective way to divert carbon flux into isobutanol biosynthesis. Concurrently, recombinant strains showed diminishing ethanol production with increasing tetracycline concentrations used for induction and isobutanol production (Fig. 6c). For instance, the isobutanol production of ZMQ3-A4 reached a titer of 4.01 ± 0.06 g/L, which was four times of that without tetracycline induction, while ethanol production in ZMQ3-A4 decreased to 10.93 ± 0.99 g/L, 50% of ZMQ3-A4 without tetracycline induction (Fig. 6c). Therefore, our results indicated that the overexpression of the synthetic operon, als-ilvC-ilvD and kdcA, could enhance isobutanol production by diverting carbon flux from ethanol biosynthesis to isobutanol biosynthesis pathway.
Growth of the recombinant strain ZMQ3-A4 with the highest isobutanol titer was further examined in this study. The results showed that although isobutanol titer increased gradually, the growth rates of ZMQ3-A4 dropped with the increase of tetracycline inducer concentrations (Fig. 6d). As discussed above, the growth rate of Z. mobilis with the supplementation of 4 g/L isobutanol (0.47 ± 0.01) was almost the same as that without isobutanol supplementation (0.50 ± 0.00). Thus, the maximum isobutanol titer produced in this study by ZMQ3-A4 is not likely to affect cellular growth significantly. Together with the fact that the tetracycline concentrations used to induce the synthetic operon als-ilvC-ilvD does not affect the normal growth of Z. mobilis, slight growth inhibition in the ZMQ3-A4 recombinant strain under these highly inducing tetracycline concentrations is likely due to the protein production burden, precursor competition, and electron balancing resulting from the increased expression of isobutanol biosynthesis pathway genes, similar to that observed in a 2,3-butanediol production recombinant strain previously reported .
Although the recombinant strain ZMQ3-A4 had the highest isobutanol titers among three recombinant strains ZMQ3-A2, ZMQ3-A3, and ZMQ3-A4 under each tetracycline induction conditions (Fig. 6C), ZMQ3-A4 had higher isobutanol yield (%) with the tetracycline induction at concentrations of 0.2 and 1.0 μg/mL than those of ZMQ3-A2 and ZMQ3-A3 (Additional file 1: Table S1). The difference between ZMQ3-A3 and ZMQ3-A4 is als gene while ZMQ3-A3 used als gene from B. licheniformis and ZMQ3-A4 uses als gene from B. subtilis (Fig. 5a). The impact of heterologous pathway and different heterologous pathway genes on endogenous metabolic pathways and regulatory networks as well as the compatibility between heterologous pathways and chassis cells should also be investigated to help improve the titer, yield, and productivity of isobutanol production.
In addition, although our study gradually increased the isobutanol production through metabolic engineering with a titer up to 4.01 g/L, which is equal to or higher than the titer using other model species such as yeast S. cerevisiae (2.09 g/L), B. subtilis (2.6 g/L), Ralstonia eutropha (0.85 g/L), and S. elongatus (0.45 g/L), it is still far less than the titers achieved using E. coli (50 g/L) and C. glutamicum (72.69 g/L) [50, 54]. Significant effort is still needed to further improve isobutanol tolerance and increase isobutanol titer, yield, and productivity including in situ product removal by gas stripping, knockout of pyruvate decarboxylase (Pdc) to redirect carbon flux from ethanol production into isobutanol production, as well as mutagenesis strategies such as ALE and atmospheric and room temperature plasma (ARTP) mutagenesis [55, 56].
The effect of oxygen on isobutanol production
As discussed above, although significant progress was made for isobutanol production through metabolic engineering in different microorganisms, nearly all of them are aerobic microorganisms producing isobutanol under aerobic conditions even though E. coli and S. cerevisiae were recently engineered for anaerobic isobutanol production [7, 57]. Since Z. mobilis is a facultative anaerobic ethanologen, we investigated the impact of the amount of oxygen on isobutanol production using shake flasks containing different medium volumes of 20, 50, or 80% of the capacity of the flask similar to our previous work for 2,3-butanediol production . Our results showed that isobutanol production was affected by the oxygenation of the medium in the shake flask. More isobutanol was produced in shake flasks with a higher medium volume which contains less oxygen due to poorer mixing (Fig. 7).
Correlated with the low isobutanol production in the 20% volume condition in shake flask fermentation, glucose consumption and culture growth were impeded with less than 4.22 g/L ethanol produced after consuming almost all of the glucose (Additional file 2: Fig. S1A, Additional file 3: Table S2). In the 50% and 80% medium volume conditions, there was no significant change in cellular growth. However, when same concentration of tetracycline inducer was used, the titers of both ethanol and isobutanol under 80% medium volume condition were more than those under 50% medium volume condition (Additional file 2: Fig. S1B, C; Additional file 3: Table S2).
Concurrent with the reduced glucose utilization and cellular growth in the 20% medium volume condition, the byproducts of glycerol, acetate, and acetoin were increased (Additional file 2: Fig. S1D, Additional file 3: Table S2) consistent with our previous study for Z. mobilis in aerobic and anaerobic conditions . Moreover, when the same concentrations of tetracycline were used, the productivity of almost all byproducts in the 20% medium volume condition were decreased compared to those in the 80% medium volume condition (Additional file 2: Fig. S1D–F; Additional file 3: Table S2). With the increase of fermentation medium volume, less byproducts will be produced (Additional file 2: Fig. S1D–F; Additional file 3: Table S2), which again is consistent with the results of our previous study . All these results suggested that fermentation in an anoxic condition is a better choice for isobutanol production in Z. mobilis.
A well-balanced, low NADH/NAD+ ratio is the key for efficient glycolysis and cellular growth in Z. mobilis. Our previous study indicated that growth conditions impacting oxygen dispersion such as shaking speed and medium volume affected acetoin and 2,3-BDO production, and a microaerophilic condition best suitable for 2,3-BDO production . Furthermore, the decrease of oxygen availability with the increase of flask medium volume can help sustain a more anoxic condition for efficient ethanol fermentation, which in return will produce more CO2 to retain the anoxic condition during its active exponential growth phase. On the contrary, the decrease of medium volume in the flask will result in the increase of amount of oxygen, and the competition between oxygen respiration and fermentation. To help maintain the redox balance due to the NADH oxidization under aerobic condition, more byproducts of acetoin, acetate, lactate, and glycerol might therefore be produced resulting in less ethanol and/or isobutanol production as reported in the literature [4, 12], which is same as what we observed in this study (Additional file 2: Fig. S1; Additional file 3: Table S2).
Similar to heterologous 2,3-BDO production, only one NAD+ will be regenerated from isobutanol biosynthesis compared to two NAD+ from ethanol fermentation. The reduced NAD+ generated via the heterologous isobutanol or 2,3-BDO metabolic pathway and the competition for substrate towards the production of byproducts such as glycerol may help increase the NADH/NAD+ ratio to maintain a balanced redox . However, the requirement of oxygen for efficient isobutanol production with highest isobutanol titer achieved under fermentation in an anoxic condition (Fig. 7) was different from that for heterologous 2,3-butanediol (BDO) production in Z. mobilis, where microaerophilic condition was most suitable for 2,3-BDO production . Therefore, further investigation is needed to understand the relationship among oxygen availability, growth phase, respiratory chain, NADH/NAD+ ratio, native glycolysis, and ethanol fermentation pathways for efficient isobutanol biosynthesis in Z. mobilis.
In summary, the effect of exogenous isobutanol on Z. mobilis was investigated and various recombinant strains for isobutanol production were constructed. Z. mobilis can grow with the supplementation of isobutanol up to 12 g/L, and the integration of a heterologous 2-ketoisovalerate decarboxylase gene (kdcA) is required for isobutanol production in Z. mobilis. In addition, recombinant strains containing a kdcA gene driven by the constitutive strong promoter Pgap (Pgap-kdcA), as well as a synthetic operon Ptet-als-ilvC-ilvD containing a heterologous als and native ilvC and ilvD genes driven by Ptet were shown to be able to divert carbon flux from ethanol production into isobutanol biosynthesis. These recombinant strains produced a maximum isobutanol titer up to 4.01 g/L accompanied by a corresponding decrease in ethanol production. This work also provides a strategy for harnessing a heterologous valine metabolic pathway for the production of other pyruvate-derived biochemicals in Z. mobilis.
Strains, vectors, and media
The plasmids and strains used in this study are listed in Tables 1 and 2, respectively. E. coli DH5α was used for plasmid construction and E. coli Trans110 (rpsL (StrR) thr leu thi-1 lacY galK galT ara tonA tsx dam dcm supE44 Δ(lac-proAB)/F′ [traD36proAB lacIq lacZΔM15]) was used as the host for plasmid demethylation. Z. mobilis ZM4 was the parent strain for genetic modifications. All E. coli strains were cultured in Luria–Bertani medium (LB, 10 g/L tryptone, 5 g/L yeast extract, 10 g/L NaCl) at 37 °C and Z. mobilis strains were cultured in rich medium (RM, 10 g/L yeast extract, 45 g/L glucose, 2 g/L KH2PO4) at 30 °C. When required, antibiotics were used at the following final concentrations: spectinomycin (100 μg/mL) and chloramphenicol (50 μg/mL).
DNA manipulation techniques
For all plasmid constructions, the steps are as follows. Primers were designed to contain 15–20 nucleotides (nts) overlapping regions with adjacent DNA fragments. PCR products amplified by primer pairs were separated by gel electrophoresis, followed by column purification, and subsequently quantified using a NanoDrop spectrophotometer (NanoDrop Technologies, Wilmington, DE, USA). Fragments and vectors were mixed in a molar ratio of 3:1, 0.5 U T5 exonuclease (NEB, USA), and 0.5 μL buffer 4 (NEB, USA) were added in a final volume of 5 μL. All regents were mixed and incubated on ice for 5 min. The DNA reaction was added to chemically competent E. coli cells, incubated on ice for 30 min, heat shocked for 45 s at 42 °C, and held on ice for 2 min. Subsequently, 100 μL of NZY medium (yeast extract 5.0 g/L, NaCl 5 g/L, MgCl2 1.2 g/L, MgSO4 1.5 g/L, glucose 3.6 g/L, casein enzymatic hydrolysate NZ amine® 10 g/L), was added to the mixture and recovered for at least 1 h at 37 °C with shaking (250 rpm).
Cells were plated on LB agar plates containing appropriate antibiotics. Recombinants were selected by colony PCR and confirmed by Sanger sequencing (TsingKe Biological Technology, Wuhan, China). The universal primers 15A-fwd/rev or M13-fwd/rev was used for colony PCR to check the insert size. Colonies containing correct plasmids with expected PCR product length through colony PCR screenings were cultivated in LB medium containing appropriate antibiotics for plasmid extraction, which was further Sanger sequencing confirmed (Tsingke Biological Technology, Wuhan, China).
Genetic modification of Z. mobilis was based on homologous recombination using a pUC57 suicide vector, which is unstable due to the lack of Z. mobilis replicative elements. The gene expression cassette flanking 1-kb upstream and 1-kb downstream of editing sites was assembled into the pUC57 vector. The customized specific plasmid was then transferred into Z. mobilis competent cells. Gene insertions were screened by colony PCR with the primer pair upstream-F and downstream-R, and further confirmed by Sanger sequencing (Tsingke Biological Technology, Wuhan, China).
Electroporation transformation and strain selection
Electrocompetent Z. mobilis was prepared as described with slight modifications . Briefly, Z. mobilis and its derivates were revived from glycerol stock on an RM plate. Then a single colony was picked and inoculated into a 10-mL screw-capped or disposable culture tube at 30 °C, statically overnight. Five milliliters of this overnight culture were then transferred to 500-mL RMG in a capped bottle with an initial OD600nm of 0.025 to 0.03 and cultured at 30 °C until early/mid log phase (OD600nm of 0.4 to 0.6). The culture was chilled on ice for 10 min, and cells were collected at 4 °C, 4000 rpm, 10 min. Cells were resuspended and washed with pre-chilled water once, resuspended, and washed with pre-chilled 10% (v/v) glycerol twice. Finally, cell pellets were resuspended in 10% glycerol at a concentration approximately 1000-fold higher than the starting culture. Competent cells (100 μL) were transferred into 1.5-mL Eppendorf tubes and stored at − 80 °C for later use.
For each electroporation transformation, 50 μL of the competent cells were mixed with 0.5 ~ 5 μg DNA. In 0.1-cm electroporation cuvettes, the cells and plasmid DNA were electroporated (1.6 kV, 25 μF, and 200 ohms) using a Bio-Rad Gene Pulser. The electroporated cells were transferred to 1 mL of mating medium (glucose 50 g/L, yeast extract 10 g/L, tryptone 5 g/L, (NH4)2SO4 2.5 g/L, K2HPO4 0.2 g/L, 1 mM MgSO4), and recovered at 30 °C for 8 to 12 h. Cells were then spread on RM agar plates containing appropriate antibiotics and incubated at 30 °C for 2 to 3 d to isolate single colonies. Since the restriction modification systems in Z. mobilis can reduce the transformation efficiency , the plasmid was transformed into a methylation-deficient E. coli (Trans110) for efficient transformation. The universal primers 15A-fwd/rev were used for colony PCR to check the insert size. Colonies with correct plasmids were cultivated in RMG medium containing appropriate antibiotics for preservation.
Growth curve analysis using Bioscreen C
Cell growth was monitored by measuring the cell OD values using a Bioscreen C high-throughput growth measurement instrument (Bioscreen C MBR, Helsinki, Finland). Three technical replicates were used for each condition. According to previous work , Z. mobilis was rather sensitive to 2% butanol and reached only 20% of its growth rate without butanol supplementation. Moreover, E. coli cannot tolerate 2% isobutanol (http://2012.igem.org/Team:NCTU_Formosa/Modeling). So, we chose six isobutanol concentrations (0, 4, 8, 12, 16, 20 g/L) to examine the isobutanol toxicity on Z. mobilis. Each well of the Bioscreen C plate contained 300 μL bacterium suspension with an initial OD600nm value of ca. 0.05.
Batch fermentation in shake flasks
Growth curves of Z. mobilis ZM4 and its derivates were determined as follows. Strains revived from glycerol stock were inoculated into 5-mL RM media containing appropriate antibiotics and grown overnight without shaking at 30 °C as the seed culture. The seed culture was then transferred into 100-mL shake flasks with 80 mL medium at an initial OD600nm of 0.1. Strains were cultured in shake flakes (30 °C, 100 rpm). Most experiments were performed with medium at 80% of the shake flask volume except for the experiment to investigate the impact of oxygen on isobutanol production using different medium volumes of 20, 50, and 80% of flask volume controlling the amount of dissolved oxygen. For example, the 100-mL shake flasks containing 80 mL RMG (80%) was considered as the least oxygenated anoxic condition, while 100-mL shake flasks containing 20 mL RMG (20%) were regarded as aerobic conditions. Flasks were capped with gas-permeable membrane. Samples from the shake flasks were taken at various time points and the biomass was evaluated by determination of optical density (OD600nm) using a spectrometer. Three technical replicates were used for each condition.
High‑performance liquid chromatography (HPLC) analysis
Samples from the shake flasks were centrifuged at 13,000 rpm for 2 min at 4 °C and then supernatants were filtered through a 0.2-μm syringe filter into HPLC vials. Concentrations of isobutanol, glucose, and ethanol in the supernatant were then determined by an HPLC system (HPLC Prominence, Shimadzu, Japan) equipped with a Bio-Rad Aminex HPX-87H column (Bio-Rad, Hercules, CA, USA) and a refractive index detector (RID). The column temperature was set at 60 °C and 5 mM H2SO4 solution was used as the mobile phase with a flow rate of 0.5 mL/min.
Availability of data and materials
The authors declare that all the data supporting the findings of this study are available within the paper and its Supplementary Information files or are available from the corresponding author on request.
high-performance liquid chromatography
He MX, Wu B, Qin H, Ruan ZY, Tan FR, Wang JL, Shui ZX, Dai LC, Zhu QL, Pan K, et al. Zymomonas mobilis: a novel platform for future biorefineries. Biotechnol Biofuels. 2014;7:101.
Wang X, He Q, Yang Y, Wang J, Haning K, Hu Y, Wu B, He M, Zhang Y, Bao J, et al. Advances and prospects in metabolic engineering of Zymomonas mobilis. Metab Eng. 2018;50:57–73.
Lee SK, Chou H, Ham TS, Lee TS, Keasling JD. Metabolic engineering of microorganisms for biofuels production: from bugs to synthetic biology to fuels. Curr Opin Biotechnol. 2008;19(6):556–63.
Yang S, Mohagheghi A, Franden MA, Chou YC, Chen X, Dowe N, Himmel ME, Zhang M. Metabolic engineering of Zymomonas mobilis for 2,3-butanediol production from lignocellulosic biomass sugars. Biotechnol Biofuels. 2016;9(1):189.
Peralta-Yahya PP, Zhang F, del Cardayre SB, Keasling JD. Microbial engineering for the production of advanced biofuels. Nature. 2012;488(7411):320–8.
Zhang F, Rodriguez S, Keasling JD. Metabolic engineering of microbial pathways for advanced biofuels production. Curr Opin Biotechnol. 2011;22(6):775–83.
Chen X, Nielsen KF, Borodina I, Kielland-Brandt MC, Karhumaa K. Increased isobutanol production in Saccharomyces cerevisiae by overexpression of genes in valine metabolism. Biotechnol Biofuels. 2011;4:21.
Blombach B, Riester T, Wieschalka S, Ziert C, Youn JW, Wendisch VF, Eikmanns BJ. Corynebacterium glutamicum tailored for efficient isobutanol production. Appl Environ Microbiol. 2011;77(10):3300–10.
Chen CT, Liao JC. Frontiers in microbial 1-butanol and isobutanol production. FEMS Microbiol Lett. 2016;363(5):fnw020.
Yang S, Fei Q, Zhang Y, Contreras LM, Utturkar SM, Brown SD, Himmel ME, Zhang M. Zymomonas mobilis as a model system for production of biofuels and biochemicals. Microb Biotechnol. 2016;9(6):699–717.
Panesar PS, Marwaha SS, Kennedy JF. Zymomonas mobilis: an alternative ethanol producer. J Chem Technol Biotechnol. 2006;81(4):623–35.
Yang S, Tschaplinski TJ, Engle NL, Carroll SL, Martin SL, Davison BH, Palumbo AV, Rodriguez M Jr, Brown SD. Transcriptomic and metabolomic profiling of Zymomonas mobilis during aerobic and anaerobic fermentations. BMC Genomics. 2009;10:34.
Zhang M, Eddy C, Deanda K, Finkelstein M, Picataggio S. Metabolic engineering of a pentose metabolism pathway in ethanologenic Zymomonas mobilis. Science. 1995;267(5195):240–3.
König S. Subunit structure, function and organisation of pyruvate decarboxylases from various organisms. Biochim et Biophys Acta (BBA) Protein Struct Mol Enzymol. 1998;1385(2):271–86.
Yang S, Vera JM, Grass J, Savvakis G, Moskvin OV, Yang Y, McIlwain SJ, Lyu Y, Zinonos I, Hebert AS, et al. Complete genome sequence and the expression pattern of plasmids of the model ethanologen Zymomonas mobilis ZM4 and its xylose-utilizing derivatives 8b and 2032. Biotechnol Biofuels. 2018;11:125.
Xia J, Yang Y, Liu C-G, Yang S, Bai FW. Engineering Zymomonas mobilis for robust cellulosic ethanol production. Trends Biotechnol. 2019:37:960–72.
He MX, Wu B, Shui ZX, Hu QC, Wang WG, Tan FR, Tang XY, Zhu QL, Pan K, Li Q, et al. Transcriptome profiling of Zymomonas mobilis under ethanol stress. Biotechnol Biofuels. 2012;5(1):75.
Seo JS, Chong H, Park HS, Yoon KO, Jung C, Kim JJ, Hong JH, Kim H, Kim JH, Kil JI, et al. The genome sequence of the ethanologenic bacterium Zymomonas mobilis ZM4. Nat Biotechnol. 2005;23(1):63–8.
Yang S, Pan C, Hurst GB, Dice L, Davison BH, Brown SD. Elucidation of Zymomonas mobilis physiology and stress responses by quantitative proteomics and transcriptomics. Front Microbiol. 2014;5:246.
Yang S, Pan C, Tschaplinski TJ, Hurst GB, Engle NL, Zhou W, Dam P, Xu Y, Rodriguez M Jr, Dice L, et al. Systems biology analysis of Zymomonas mobilis ZM4 ethanol stress responses. PLoS ONE. 2013;8(7):e68886.
Zhao N, Bai Y, Zhao XQ, Yang ZY, Bai FW. Draft genome sequence of the flocculating Zymomonas mobilis strain ZM401 (ATCC 31822). J Bacteriol. 2012;194(24):7008–9.
Yang S, Pappas KM, Hauser LJ, Land ML, Chen GL, Hurst GB, Pan C, Kouvelis VN, Typas MA, Pelletier DA, et al. Improved genome annotation for Zymomonas mobilis. Nat Biotechnol. 2009;27(10):893–4.
Widiastuti H, Kim JY, Selvarasu S, Karimi IA, Kim H, Seo JS, Lee DY. Genome-scale modeling and in silico analysis of ethanologenic bacteria Zymomonas mobilis. Biotechnol Bioeng. 2011;108(3):655–65.
Pentjuss A, Odzina I, Kostromins A, Fell DA, Stalidzans E, Kalnenieks U. Biotechnological potential of respiring Zymomonas mobilis: a stoichiometric analysis of its central metabolism. J Biotechnol. 2013;165(1):1–10.
Jia X, Wei N, Wang T, Wang H. Use of an EZ-Tn5-based random mutagenesis system to create a Zymomonas mobilis with significant tolerance to heat stress and malnutrition. J Ind Microbiol Biotechnol. 2013;40(8):811–22.
Kerr AL, Jeon YJ, Svenson CJ, Rogers PL, Neilan BA. DNA restriction-modification systems in the ethanologen, Zymomonas mobilis ZM4. Appl Microbiol Biotechnol. 2011;89(3):761–9.
Zhang X, Wang T, Zhou W, Jia X, Wang H. Use of a Tn5-based transposon system to create a cost-effective Zymomonas mobilis for ethanol production from lignocelluloses. Microb Cell Fact. 2013;12:41.
Yang Y, Shen W, Huang J, Li R, Xiao Y, Wei H, Chou YC, Zhang M, Himmel ME, Chen S, et al. Prediction and characterization of promoters and ribosomal binding sites of Zymomonas mobilis in system biology era. Biotechnol Biofuels. 2019;12:52.
Zheng Y, Han J, Wang B, Hu X, Li R, Shen W, Ma X, Ma L, Yi L, Yang S, et al. Characterization and repurposing of the endogenous Type I-F CRISPR-Cas system of Zymomonas mobilis for genome engineering. Nucleic Acids Res. 2019;47:11461–75.
Yang Y, Rong Z, Song H, Yang X, Li M, Yang S. Identification and characterization of ethanol inducible promoters of Zymomonas mobilis based on omics data and dual reporter-gene system. Biotechnol Appl Biochem. 2019;. https://doi.org/10.1002/bab.1838.
Shen W, Zhang J, Geng B, Qiu M, Hu M, Yang Q, Bao W, Xiao Y, Zheng Y, Peng W, et al. Establishment and application of a CRISPR-Cas12a assisted genome-editing system in Zymomonas mobilis. Microb Cell Fact. 2019;18(1):162.
Yang Y, Hu M, Tang Y, Geng B, Qiu M, He Q, Chen S, Wang X, Yang S. Progress and perspective on lignocellulosic hydrolysate inhibitor tolerance improvement in Zymomonas mobilis. Bioresour Bioprocess. 2018;5(1):6.
Atsumi S, Hanai T, Liao JC. Non-fermentative pathways for synthesis of branched-chain higher alcohols as biofuels. Nature. 2008;451(7174):86–9.
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(1–2):32–7.
Siripong W, Wolf P, Kusumoputri TP, Downes JJ, Kocharin K, Tanapongpipat S, Runguphan W. Metabolic engineering of Pichia pastoris for production of isobutanol and isobutyl acetate. Biotechnol Biofuels. 2018;11:1.
Li S, Wen J, Jia X. Engineering Bacillus subtilis for isobutanol production by heterologous Ehrlich pathway construction and the biosynthetic 2-ketoisovalerate precursor pathway overexpression. Appl Microbiol Biotechnol. 2011;91(3):577–89.
Smith KM, Cho K-M, Liao JC. Engineering Corynebacterium glutamicum for isobutanol production. Appl Microbiol Biotechnol. 2010;87(3):1045–55.
Lin PP, Rabe KS, Takasumi JL, Kadisch M, Arnold FH, Liao JC. Isobutanol production at elevated temperatures in thermophilic Geobacillus thermoglucosidasius. Metab Eng. 2014;24:1–8.
Miao R, Xie H. F MH, Lindblad P: Protein engineering of alpha-ketoisovalerate decarboxylase for improved isobutanol production in Synechocystis PCC 6803. Metab Eng. 2018;47:42–8.
Miao R, Xie H, Lindblad P. Enhancement of photosynthetic isobutanol production in engineered cells of Synechocystis PCC 6803. Biotechnol Biofuels. 2018;11:267.
Varman AM, Xiao Y, Pakrasi HB, Tang YJ. Metabolic engineering of Synechocystis sp. strain PCC 6803 for isobutanol production. Appl Environ Microbiol. 2013;79(3):908–14.
Atsumi S, Wu TY, Eckl EM, Hawkins SD, Buelter T, Liao JC. Engineering the isobutanol biosynthetic pathway in Escherichia coli by comparison of three aldehyde reductase/alcohol dehydrogenase genes. Appl Microbiol Biotechnol. 2010;85(3):651–7.
Baez A, Cho KM, Liao JC. High-flux isobutanol production using engineered Escherichia coli: a bioreactor study with in situ product removal. Appl Microbiol Biotechnol. 2011;90(5):1681–90.
Ghosh IN, Martien J, Hebert AS, Zhang Y, Coon JJ, Amador-Noguez D, Landick R. OptSSeq explores enzyme expression and function landscapes to maximize isobutanol production rate. Metab Eng. 2019;52:324–40.
Atsumi S, Higashide W, Liao JC. Direct photosynthetic recycling of carbon dioxide to isobutyraldehyde. Nat Biotechnol. 2009;27:1177.
Miao R, Liu X, Englund E, Lindberg P, Lindblad P. Isobutanol production in Synechocystis PCC 6803 using heterologous and endogenous alcohol dehydrogenases. Metab Eng Commun. 2017;5:45–53.
Buijs NA, Siewers V, Nielsen J. Advanced biofuel production by the yeast Saccharomyces cerevisiae. Curr Opin Chem Biol. 2013;17(3):480–8.
Shi A, Zhu X, Lu J, Zhang X, Ma Y. Activating transhydrogenase and NAD kinase in combination for improving isobutanol production. Metab Eng. 2013;16:1–10.
Liu Z, Liu P, Xiao D, Zhang X. Improving isobutanol production in metabolically engineered Escherichia coli by co-producing ethanol and modulation of pentose phosphate pathway. J Ind Microbiol Biotechnol. 2016;43(6):851–60.
Wess J, Brinek M, Boles E. Improving isobutanol production with the yeast Saccharomyces cerevisiae by successively blocking competing metabolic pathways as well as ethanol and glycerol formation. Biotechnol Biofuels. 2019;12:173.
Morita K, Nomura Y, Ishii J, Matsuda F, Kondo A, Shimizu H. Heterologous expression of bacterial phosphoenol pyruvate carboxylase and Entner–Doudoroff pathway in Saccharomyces cerevisiae for improvement of isobutanol production. J Biosci Bioeng. 2017;124(3):263–70.
Noda S, Mori Y, Oyama S, Kondo A, Araki M, Shirai T. Reconstruction of metabolic pathway for isobutanol production in Escherichia coli. Microb Cell Fact. 2019;18(1):124.
Yang S, Pelletier DA, Lu TY, Brown SD. The Zymomonas mobilis regulator hfq contributes to tolerance against multiple lignocellulosic pretreatment inhibitors. BMC Microbiol. 2010;10(1):1–11.
Bai W, Geng W, Wang S, Zhang F. Biosynthesis, regulation, and engineering of microbially produced branched biofuels. Biotechnol Biofuels. 2019;12:84.
Shui ZX, Qin H, Wu B, Ruan ZY, Wang LS, Tan FR, Wang JL, Tang XY, Dai LC, Hu GQ, et al. Adaptive laboratory evolution of ethanologenic Zymomonas mobilis strain tolerant to furfural and acetic acid inhibitors. Appl Microbiol Biotechnol. 2015;99(13):5739–48.
Gu C, Wang G, Mai S, Wu P, Wu J, Wang G, Liu H, Zhang J. ARTP mutation and genome shuffling of ABE fermentation symbiotic system for improvement of butanol production. Appl Microbiol Biotechnol. 2017;101(5):2189–99.
Trinh CT, Li J, Blanch HW, Clark DS. Redesigning Escherichia coli metabolism for anaerobic production of isobutanol. Appl Environ Microbiol. 2011;77(14):4894–904.
Knoshaug EP, Zhang M. Butanol tolerance in a selection of microorganisms. Appl Biochem Biotechnol. 2009;153(1–3):13–20.
This work was authored in part by the National Renewable Energy Laboratory, operated by Alliance for Sustainable Energy, LLC, for the US Department of Energy (DOE) under Contract No. DE-AC36-08GO28308. The views expressed in the article do not necessarily represent the views of the DOE or the US Government. The US Government retains and the publisher, by accepting the article for publication, acknowledges that the US Government retains a nonexclusive, paid-up, irrevocable, worldwide license to publish or reproduce the published form of this work, or allow others to do so, for US Government purposes.
This work was supported by the National Key Research and Development Program of China (2018YFA0900300), National Science Foundation of China (21978071 and U1932141), and the Technical Innovation Special Fund of Hubei Province (2019AHB055 and 2018ACA149). We also acknowledge the support from State Key Laboratory of Biocatalysis and Enzyme Engineering. Funding was also provided by the US Department of Energy, Office of Energy Efficiency and Renewable Energy, Bioenergy Technologies Office under Contract DE-AC36–08GO28308 with the National Renewable Energy Laboratory.
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Additional file 1: Table S1. The isobutanol yield relative to the maximum theoretical yields (%) for ZMQ3-A2, ZMQ3-A3, and ZMQ3-A4 strains with the induction of tetracycline at concentrations of 0, 0.2 and 1.0 μg/mL (Tc 0, Tc 0.2, and Tc 1.0, respectively) was calculated based on the information of glucose consumed (Gluc) and the production of isobutanol (Iso) and ethanol (Eth) at the time point when most glucose was consumed up and the production of isobutanol and ethanol was the highest (h). Theoretical Isobutanol Titer (g/L) is the amount of isobutanol that can be produced from all glucose consumed, which was calculated based on the formula: Theoretical Isobutanol Titer = Glucose Consumed/180.156 (MW of Glucose)*74.122 (MW of Isobutanol). Percentage of theoretical isobutanol maximum yield (Isobutanol yield, %) was then calculated based on the isobutanol produced/Theoretical Isobutanol Titer*100%.
Additional file 2: Figure S1. Cell growth, glucose consumption, ethanol and byproduct production of Z. mobilis recombinant strain ZMQ3-A4 in flask with different volume of RMG5 medium by the tetracycline induction at different concentrations of 0, 0.2, and 1 μg/mL. Cell growth, glucose (Glu) consumption, and ethanol (Eth) production of ZMQ3-A4 by the tetracycline induction at different concentrations in flask with a volume of medium at 20% (A), 50% (B), and 80% (C), as well as the production of byproducts of glycerol, acetoin, and acetate in flask with a volume of medium at 20% (D), 50% (E), and 80% (F), respectively. Tc 0, Tc 0.2 and Tc 1 represented the tetracycline concentrations of 0, 0.2, and 1.0 μg/mL that was added into the medium once from the beginning of the experiment, respectively. The results shown are the mean of two technical replicate flasks and the error bars represent standard deviations.
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Qiu, M., Shen, W., Yan, X. et al. Metabolic engineering of Zymomonas mobilis for anaerobic isobutanol production. Biotechnol Biofuels 13, 15 (2020). https://doi.org/10.1186/s13068-020-1654-x
- Zymomonas mobilis
- Metabolic engineering
- Pyruvate-derived biochemicals
- 2-Ketoisovalerate decarboxylase (Kdc)