- Open Access
Engineering Corynebacterium glutamicum for the production of 2,3-butanediol
© Radoš et al. 2015
Received: 7 July 2015
Accepted: 18 October 2015
Published: 29 October 2015
2,3-Butanediol is an important bulk chemical with a wide range of applications. In bacteria, this metabolite is synthesised from pyruvate via a three-step pathway involving α-acetolactate synthase, α-acetolactate decarboxylase and 2,3-butanediol dehydrogenase. Thus far, the best producers of 2,3-butanediol are pathogenic strains, hence, the development of more suitable organisms for industrial scale fermentation is needed. Herein, 2,3-butanediol production was engineered in the Generally Regarded As Safe (GRAS) organism Corynebacterium glutamicum. A two-stage fermentation process was implemented: first, cells were grown aerobically on acetate; in the subsequent production stage cells were used to convert glucose into 2,3-butanediol under non-growing and oxygen-limiting conditions.
A gene cluster, encoding the 2,3-butanediol biosynthetic pathway of Lactococcus lactis, was assembled and expressed in background strains, C. glutamicum ΔldhA, C. glutamicum ΔaceEΔpqoΔldhA and C. glutamicum ΔaceEΔpqoΔldhAΔmdh, tailored to minimize pyruvate-consuming reactions, i.e., to prevent carbon loss in lactic, acetic and succinic acids. Producer strains were characterized in terms of activity of the relevant enzymes in the 2,3-butanediol forming pathway, growth, and production of 2,3-butanediol under oxygen-limited conditions. Productivity was maximized by manipulating the aeration rate in the production phase. The final strain, C. glutamicum ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB,Ptuf butA), under optimized conditions produced 2,3-butanediol with a 0.66 mol mol−1 yield on glucose, an overall productivity of 0.2 g L−1 h−1 and a titer of 6.3 g L−1.
We have successfully developed C. glutamicum into an efficient cell factory for 2,3-butanediol production. The use of the engineered strains as a basis for production of acetoin, a widespread food flavour, is proposed.
Concern over exhaustion of fossil fuel resources, emission of CO2 linked with petroleum-derived products, and accumulation of non-degradable synthetic polymers urged the development of environmentally friendly processes for production of chemicals. A solution offered by the rising field of white biotechnology is to produce chemical building blocks by microbial fermentation of sugars derived from renewable biomass .
2,3-Butanediol (2,3-BD) is an important chemical used in the production of plasticizers and fumigants, as an antifreeze agent, a fuel and octane booster, among other applications . The range is still expanding and the market size is expected to reach 74 kilo tons by 2018 . Significantly, the 2,3-BD derivative, 1,3-butanediene, can be used in synthetic rubber production, while 2-butanone (methyl ethyl ketone) is a fuel additive and solvent for resins and lacquers. Additionally, ester-derivatives are used in the pharmaceutical and cosmetics industries . The world annual market for 2,3-BD derivatives is estimated at around $43 billion .
Thus far, the best producers of 2,3-BD are pathogenic strains, such as Klebsiella pneumoniae, Klebsiella oxytoca, Enterobacter aerogenes, and Serratia marcescens [7–10], hence, a considerable research effort has been directed to the development of more suitable organisms for industrial scale fermentation. Lactococcus lactis, Bacillus subtilis, Paenibacillus polymyxa, Saccharomyces cerevisiae and Escherichia coli have been used for this purpose, but the low production efficiency or complex nutritional requirements of the engineered strains make the overall process unsatisfactory [11–15]. Therefore, the search goes on for more appropriate host strains and more efficient fermentation processes. A few years ago, some of us engineered L. lactis for the production of 2,3-BD by overexpression of two endogenous genes (als, butA) ; theoretical product yields were reached, but the fastidious nutritional requisites of this bacterium precludes its utilization as an industrial producer of bulk chemicals.
In this work, we selected Corynebacterium glutamicum as an industrially established host strain and aimed to develop an efficient 2,3-BD producer. C. glutamicum is an important industrial microorganism, widely known for the million-ton scale production of l-glutamate and l-lysine . Therefore, the existing knowledge of the industrial fermentation of this bacterium could be exploited for the production of bulk chemicals, such as 2,3-BD. In addition, C. glutamicum is a facultative anaerobic organism with GRAS (Generally Regarded As Safe) status, robust (osmotolerant, phageresistant, organic solvent tolerant), extensively studied with respect to metabolism and regulation, and for which a comprehensive toolbox for genetic manipulation has been developed [17–19]. Considerable research effort has been invested in metabolic engineering of C. glutamicum, resulting in the construction of producer strains for a broad spectrum of compounds, such as biofuels (isobutanol and ethanol), polymer precursors (diaminopentane, cadaverine and putrescine), sugar alcohols (xylitol) and organic acids [20–29]. As a result of this research endeavour, platform strains of C. glutamicum have been established. More specifically, strains deficient in l-lactate dehydrogenase (LDH, encoded by ldhA) have been proven to be a useful starting point for strain development since deletion of the ldhA gene eliminates l-lactate formation, concomitantly increasing NADH availability [27, 29]. In addition, strains deficient in the aceE-encoded E1 subunit of the pyruvate dehydrogenase complex (PDHC) were also shown to be suitable hosts for the production of pyruvate and pyruvate-derived products, l-valine, l-lysine, 2-ketoisovalerate, succinate and isobutanol (reviewed in ). Typically, PDHC-deficient strains are unable to grow on glucose as sole carbon source unless the medium is supplemented with acetate or ethanol [31, 32]. However, in the absence of the latter substrates, C. glutamicum ΔaceE remains metabolically active and converts glucose to pyruvate, l-alanine and l-valine under aerobic conditions . Combined activities of pyruvate:quinone oxidoreductase, acetate kinase and phosphotransacetylase (Fig. 1) do not provide sufficient acetyl-CoA to replace the PDHC reaction in glucose containing medium, however, deletion of the respective pqo gene was shown to be beneficial for the production of pyruvate and its derived products l-valine and 2-ketoisovalerate [33, 34]. In this framework, we constructed and tested three strains as potential hosts for efficient 2,3-BD production. In addition to C. glutamicum ΔldhA, and C. glutamicum ΔaceEΔpqoΔldhA, designed to minimize lactate and acetate formation, a third strain, C. glutamicum ΔaceEΔpqoΔldhAΔmdh, was constructed with an extra deletion of the malate dehydrogenase gene to reduce succinate formation (Fig. 1). In these strains we expressed als, aldB, butA from L. lactis and devised a two-stage process for efficient production of 2,3-BD. In the first stage cells were grown aerobically on acetate or glucose for biomass formation; in the second stage (production stage), biomass was used to convert glucose into 2,3-BD under non-growing and oxygen-limiting conditions.
Design of a synthetic pathway for 2,3-BD and functional analysis
Bacterial strains and plasmids used in this study
E. coli DH5α
Plasmid-free E. coli
C. glutamicum ATCC13032
C. glutamicum ΔldhA
ATCC13032 with deletion of lactate dehydrogenase gene ldhA
C. glutamicum ΔaceEΔpqoΔldhA
ATCC13032 with deletions of the genes for the E1 subunit of pyruvate dehydrogenase complex, the pyruvate:quinone oxidoreductase and the lactate dehydrogenase
C. glutamicum ΔaceEΔpqo
ATCC13032 with deletions of the genes for the E1 subunit of pyruvate dehydrogenase complex, the pyruvate:quinone oxidoreductase, lactate dehydrogenase and malate dehydrogenase
C. glutamicum ΔaceEΔpqo
C. glutamicum ΔaceEΔpqoΔldhA harboring plasmid pEKEx2
C. glutamicum ΔldhA (pEKEx2)
C. glutamicum ΔldhA harboring plasmid pEKEx2
C. glutamicum ΔaceEΔpqo
C. glutamicum ΔaceEΔpqoΔldhAΔmdh harboring plasmid pEKEx2
C. glutamicum ΔldhA (pEKEx2- als,aldB,butA)
C. glutamicum ΔldhA harboring plasmid pEKEx2 als,aldB,butA
C. glutamicum ΔaceEΔpqo
C. glutamicum ΔaceEΔpqoΔldhA harboring plasmid pEKEx2-als,ald,BbutA
C. glutamicum ΔaceEΔpqo
C. glutamicum ΔaceEΔpqoΔldhAΔmdh harboring plasmid pEKEx2-als,aldB,butA
C. glutamicum ΔaceEΔpqo
ΔldhA (pEKEx2-als,aldB, Ptuf butA)
C. glutamicum ΔaceEΔpqoΔldhA harboring plasmid pEKEx2-als,aldB, Ptuf butA
C. glutamicum ΔaceEΔpqo
ΔldhAΔmdh (pEKEx2-als,aldB, Ptuf butA)
C. glutamicum ΔaceEΔpqoΔldhAΔmdh harboring plasmid pEKEx2-als,aldB, Ptuf butA
kanR from pUC4 K; P trc , lacI, pUC18 mcs, induced by addition of IPTG
pEKEx2 with cloned als from L. lactis
pEKEx2-als with cloned aldB and butA from L. lactis
pEKEx2-als,aldB, Ptuf butA
pEKEx2-als with cloned aldB and Ptuf-butA from L. lactis
Overexpression and specific activities of enzymes for the synthesis of 2,3-butanediol as determined in crude cell extracts
ALS/ALDC activity U (mg of protein)−1
BDH activity U (mg of protein)−1
ALS/ALDC over-expression (-fold)
BDH over-expression (-fold)
0.02 ± 0.00
0.66 ± 0.03
1.47 ± 0.42
1.18 ± 0.26
0.04 ± 0.00
0.20 ± 0.03
0.54 ± 0.09
0.10 ± 0.03
0.03 ± 0.01
0.24 ± 0.04
0.58 ± 0.12
0.67 ± 0.01
ΔaceEΔpqoΔldhA (pEKEx2-als,aldB, Ptuf butA)
1.42 ± 0.24
0.53 ± 0.17
0.06 ± 0.02
0.11 ± 0.04
0.43 ± 0.04
0.97 ± 0.19
ΔaceEΔpqoΔldhAΔmdh (pEKEx2-als,aldB, Ptuf butA)
0.47 ± 0.14
1.21 ± 0.01
Growth profiles of engineered strains
First, we characterized growth and biomass formation of the engineered strains in shake-flasks in 2× TY medium containing glucose or acetate (Additional file 1: Fig. S2, Table S1). The ΔaceE strains (PDHC-deficient) are unable to grow on glucose as sole carbon source, therefore, they were grown aerobically on acetate alone. Strains C. glutamicum Δldh(pEKEx2) and ΔldhA(pEKEx2-als,aldB,butA) were grown on glucose and also on acetate for comparison purposes. While the control strain C. glutamicum Δldh(pEKEx2) had similar specific growth rates when grown on glucose or acetate (0.52 ± 0.02 and 0.51 ± 0.05 h−1, respectively), ΔldhA(pEKEx2-als,aldB,butA) displayed a lower growth rate on acetate (0.46 ± 0.01 versus 0.58 ± 0.01 h−1). The pH profiles were also dependent on the substrate used for growth as glucose-grown cells presented a sharper decrease in pH at the onset of stationary phase (Additional file 1: Fig. S2). The biomass formation was fairly similar for C. glutamicum Δldh(pEKEx2) and producer strain ΔldhA(pEKEx2-als,aldB,butA) regardless of the substrate used for growth (maximal OD600 values in the range 21–24). The C. glutamicum ΔaceEΔpqoΔldhA-derived producers showed growth and pH profiles identical to those of the control strain ΔaceEΔpqoΔldhA(pEKEx2). The specific growth rate of C. glutamicum ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB,butA) was higher as compared to the control strain ΔaceEΔpqoΔldhAΔmdh(pEKEx2) (0.55 ± 0.04 vs 0.46 ± 0.01 h−1); on the other hand, the growth rate of ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB, Ptuf butA) was comparable to that of the control strain (0.44 ± 0.01 vs 0.46 ± 0.01 h−1). For all ΔaceEΔpqoΔldhA- and ΔaceEΔpqoΔldhAΔmdh-derived strains, the initial and final pH values were 7.1 and 9.2, respectively, and maximal OD600 values were in the range 15–19. In summary, cell growth was not impaired by the expression of heterologous genes (Additional file 1: Table S1), reflecting the robustness of these platform strains.
Characterization of 2,3-BD production under low-oxygen conditions
Glucose (Glc) consumption rate (GCR), molar yield and productivity of 2,3-butanediol (2,3-BD), and carbon recovery (CR) by the control and engineered C. glutamicum strains
GCR (nmol min−1 mg CDW−1)
Yield (mol 2,3-BD per mol Glc)
Productivity (nmol min−1 mg CDW−1)
2.5 ± 0.4
0.05 ± 0.00#
0.12 ± 0.01
81 ± 3
ΔldhA (pEKEx2- als,aldB,butA)*
4.4 ± 0.4
0.34 ± 0.04
1.28 ± 0.09
79 ± 9
3.0 ± 0.2
0.02 ± 0.01#
0.06 ± 0.03
77 ± 1
ΔldhA (pEKEx2- als,aldB,butA)
3.4 ± 0.4
0.27 ± 0.06
0.53 ± 0.13
82 ± 3
1.6 ± 0.3
0.22 ± 0.01#
0.30 ± 0.00
87 ± 1
5.4 ± 0.7
0.66 ± 0.05
3.55 ± 0.58
84 ± 7
ΔaceEΔpqoΔldhA (pEKEx2-als,aldB, Ptuf butA)
6.1 ± 0.1
0.61 ± 0.06
3.13 ± 0.22
87 ± 3
1.6 ± 0.3
0.34 ± 0.05#
0.53 ± 0.00
91 ± 6
6.0 ± 0.3
0.64 ± 0.09
4.34 ± 0.16
90 ± 4
ΔaceEΔpqoΔldhAΔmdh (pEKEx2-als,aldB, Ptuf butA)
6.5 ± 0.5
0.64 ± 0.10
4.25 ± 0.41
91 ± 7
The inactivation of the PDHC and PQO in the producer strain ΔaceEΔpqoΔldhA(pEKEx2-als,aldB,butA) had a drastic effect on 2,3-BD yield that increased from 0.27 ± 0.06 in ΔldhA(pEKEx2-als,aldB,butA), to 0.66 ± 0.05 mol per mol, reflecting primarily the reduction of acetate formation (from 29 mM to below 0.5 mM). Moreover, the GCR increased about 1.6-fold and there was a sevenfold increase in overall productivity. Glycerol and succinate were the major side-products (12 ± 1 and 8 ± 1 mM, respectively) (Fig. 2).
Further engineering aimed at succinate reduction (MDH inactivation by deletion of the cg2613-encoded activity), left both yield and GCR essentially unchanged while productivity was slightly improved in C. glutamicum ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB,butA) (4.3 ± 0.2 compared to 3.6 ± 0.6 nmol min−1 mg CDW−1). Strains in which the lactococcal butA gene was placed under the control of Ptuf promoter showed similar behavior to those which had this gene under Ptac control in terms of all production parameters (Table 3; Fig. 2). In summary, C. glutamicum ΔaceEΔpqoΔldhA(pEKEx2-als,aldB,butA), ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB,butA) and ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB, Ptuf butA) showed the highest yield of about 0.65 mol 2,3-BD per mol of glucose with the latter two strains exhibiting the highest productivities of about 4.3 nmol 2,3-BD per min and mg CDW (Table 3). All control strains produced optically active 2,3-BD, while only the meso-form was found as end-product of the producer strains (Fig. 2, Additional file 1: Table S3).
It is important to note that pH was not controlled during the production phase. All fermentations started at pH 7.0, but the final pH value varied as mutants exhibited different acidifying properties due to their differential ability to produce organic acids. At the end of 48 h-fermentation, pH was between 5.1 and 5.3 for ldhA-negative strains. As expected, reduction of succinate and acetate, and accumulation of neutral compounds led to higher final pH values: 6.6, 6.4, 5.7 and 6.6 for C. glutamicum ΔaceEΔpqoΔldhA(pEKEx2-als,aldB,butA), ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB,butA), ΔaceEΔpqoΔldhA(pEKEx2-als,aldB, Ptuf butA) and ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB, Ptuf butA), respectively. Earlier work has shown that a decrease in pH results in considerably lower GCR in resting cells of wild-type C. glutamicum .
Optimization of 2,3-BD production by manipulation of oxygen supply
Glucose (Glc) consumption rate (GCR), molar yield and productivity of 2,3-butanediol (2,3-BD), and carbon recovery (CR) achieved with C. glutamicum ΔaceEΔpqoΔldhA(pEKEx2-als,aldB, Ptuf butA) and C. glutamicum ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB, Ptuf butA) strains under different aeration conditions
Airflow (mL min−1)
GCR (nmol min−1 mg CDW−1)
Yield (mol 2,3-BD per mol Glc)
Productivity (nmol min−1 mg CDW−1)
ΔaceEΔpqoΔldhA (pEKEx2-als,aldB, Ptuf butA)
7.2 ± 0.6
0.44 ± 0.04
3.4 ± 0.3
89 ± 6
15.8 ± 1.7
0.57 ± 0.03
8.1 ± 0.4
91 ± 4
14.7 ± 1.1
0.36 ± 0.06
5.0 ± 0.9
83 ± 10
ΔaceEΔpqoΔldhAΔmdh (pEKEx2-als,aldB, Ptuf butA)
11.1 ± 1.0
0.52 ± 0.03
5.5 ± 0.7
85 ± 2
21.1 ± 0.8
0.66 ± 0.01
10.9 ± 1.8
90 ± 8
22.8 ± 1.6
0.46 ± 0.02
8.0 ± 0.7
78 ± 7
The wild-type C. glutamicum produces vestigial amounts of 2,3-BD . Accordingly, low levels of 2,3-BD were also found in the end-products of glucose metabolism by the control strain C. glutamicum ΔldhA(pEKEx2), the initial host in this work (Table 3). C. glutamicum was the favored candidate for 2,3-BD production given its high performance as an industrial organism and its GRAS status. Moreover, we verified that 2,3-BD has low toxicity to C. glutamicum as cell growth was not affected by 2 % 2,3-BD (data not shown). 2,3-BD producing bacteria, such as Klebsiella spp., synthesize this diol from pyruvate in a sequence of three reactions catalyzed by α-acetolactate synthase, α-acetolactate decarboxylase and butanediol dehydrogenase. In this work, we constructed an artificial operon with the three relevant genes of L. lactis and introduced this heterologous pathway into C. glutamicum (Fig. 1).
C. glutamicum is able to synthesize α-acetolactate from pyruvate via the action of the anabolic enzyme, AHAS; however, this enzyme is highly inhibited by the branched chain amino acids derived from α-acetolactate . Therefore, our engineering strategy endowed the host strain with a heterologous ALS, i.e., the catabolic enzyme from L. lactis, which is not susceptible to amino acid inhibition . The enhanced activity of ALS should also be beneficial for directing the flux towards 2,3-BD.
The second step in the biosynthetic pathway, decarboxylation of α-acetolactate into R-acetoin, is carried out by α-acetolactate decarboxylase. A homologue of this enzyme is not predicted in the genome of C. glutamicum, and indeed the ALS/ALDC activity was low in cell extracts of all control strains (Table 2). The third step, reduction of acetoin, is performed by BDH, and a relatively high activity (0.2–0.3 U(mg protein)−1) was detected in the control strains (Table 2). Actually, this is not surprising given that C. glutamicum possesses (2S,3S)-BDH, which is claimed to be absolutely stereospecific for S-acetoin . Like all known ALDCs, the enzyme from L. lactis produces exclusively R-acetoin , thus a BDH with suitable stereospecific properties needed to be included.
1H-NMR can distinguish the optically active from the meso-form of 2,3-BD (Additional file 1: Fig. S3). Control strains produced only optically active 2,3-BD (Table 3), most likely derived from diacetyl formed via spontaneous decarboxylation of α-acetolactate in the presence of oxygen. Diacetyl is then converted to 2,3-(2S,3S)-BD in two reduction reactions catalyzed by the endogenous BDH (Fig. 1). In contrast to the control strains, meso-2,3-BD was by far the main form synthesized by the producer strains, the optically active form (around 5 % of total 2,3-BD), being detected only in fermentations performed at the highest aeration rates, in agreement with the oxygen dependence of the spontaneous decarboxylation of α-acetolactate. Given that C. glutamicum lacks α-acetolactate decarboxylase, the presence of BDH in this bacterium is rather puzzling. Moreover, according to a recent study, C. glutamicum BDH is a promiscuous enzyme that besides acetoin recognizes DHA as substrate, though with a low affinity (30 mM or higher DHA concentration needed for activity) . Further work should be directed to clarify the physiological role of BDH in C. glutamicum.
The L. lactis genes (als, aldB, butA) were functionally expressed in the three host strains. The combined activity ALS/ALDC was in the range 0.4–1.4 U (mg of protein)−1 for producer strains grown on acetate, corresponding to overexpression levels of 8–31-fold. Opportunely, the heterologous activities are comparable to those of glycolytic enzymes measured in crude extracts of C. glutamicum . Overexpression of butA (encoding BDH activity) was similarly successful, yielding final BDH activity up to 1.2 U (mg of protein)−1, which confirms the suitability of using the lactococcal genes for 2,3-BD production in C. glutamicum.
The introduction of the assembled pathway in C. glutamicum ΔldhA enabled efficient redirection of the flux from pyruvate into 2,3-BD. However, the yield was relatively low (0.3 mol per mol glucose) and the two major products were succinate and acetate. Hence, the next engineering step had the objective of suppressing acetate pathways; this proved to be crucial in the by-product elimination strategy, as the 2,3-BD yield doubled in the ΔaceEΔpqoΔldhA-derived producer strains (Table 3; Fig. 5). Additional inactivation of mdh did not improve the yield significantly, but there was a slight increase in productivity (Table 3).
Curiously, the strains derived from C. glutamicum ΔaceEΔpqoΔldhAΔmdh produced substantial amounts of succinate despite the intended suppression of succinate formation via the reductive branch of the TCA cycle . The genome of C. glutamicum includes mdhB (cg0763), putatively assigned as malate/L-lactate dehydrogenase, hence this second activity may contribute to succinate formation. On the other hand, involvement of the glyoxylate shunt and/or the oxidative branch of the TCA cycle cannot be ruled out.
Glycerol was the second major side-product detected in C. glutamicum ΔaceEΔpqoΔldhA- and ΔaceEΔpqoΔldhAΔmdh-derived strains. Two pathways have been proposed for the synthesis of this polyol in C. glutamicum [42, 44]. Jojima and coworkers  proposed that under oxygen-deprivation conditions glycerol is formed through reduction of DHA by the activity of endogenous BDH. On the other hand, DHA is a product of dihydroxyacetone-phosphate (DHAP) dephosphorylation via the respective phosphatase . Therefore, endogenous BDH and DHAP phosphatase are obvious targets for inactivation in further attempts to minimize side products. In this way, the electrons that are used for glycerol formation could be directed to acetoin reduction. The elimination of BDH would also be advantageous for the stereochemical purity of the desired end-product, since the small contamination with the optically active form would vanish, though at the expense of some carbon loss in the form of diacetyl.
Under production conditions (oxygen limitation), it is anticipated that the BDH activity plays an important role in satisfying the redox balance via cofactor recycling. Further enhancement of BDH activity was attempted by including an additional promoter, but the BDH activity remained unchanged (Tables 2, 3). However, a high BDH activity would not fix the redox imbalance since the synthesis of 2,3-BD results in net production of 1 mol NADH per mol of glucose consumed, and an additional sink for the reducing power becomes mandatory. Accordingly, providing controlled amounts of oxygen significantly improved GCR and 2,3-BD productivity.
Manipulation of oxygen availability had no clear impact on 2,3-BD yield, but was crucial to increase GCR, which reached maximal values of approx. 21 nmol min−1 mg CDW−1, comparable to those of C. glutamicum strains engineered for isobutanol production . This optimization step was more effective for C. glutamicum ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB, Ptuf butA) than for ΔaceEΔpqoΔldhA(pEKEx2-als,aldB, Ptuf butA) (Table 4). The reason could be related with the different BDH activity in these two strains (Table 2). The stronger activity in C. glutamicum ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB, Ptuf butA) would pull the flux towards 2,3-BD more efficiently, with concomitant benefit on the rate of NAD+ regeneration, and hence on the GCR. Further increase in the air supply (from 10 to 20 mL min−1) had a negative impact on 2,3-BD yield, which is in conformity with the equivalent accumulation of acetoin. This shift in end-products towards compounds less reduced than 2,3-BD indicates that the competition of oxygen as an electron sink became excessive.
Thus far, Klebsiella spp., E. aerogenes and S. marcescens are the top producers of 2,3-BD (reviewed in ; see also Additional file 1: Table S5 and references therein, [47–49]), however, the pathogenicity of these strains is regarded as a disadvantage and hinders large-scale production. The best non-pathogenic producer is Paenibacillus polymyxa (72 g L−1 and about 2 g L−1 h−1), which grows in complex medium and has the drawback of producing exopolysaccharides that increase the viscosity of the fermentation broth . Engineered S. cerevisiae has a 0.29 g L−1 h−1 productivity and a yield of 0.70 mol 2,3-BD per mol glucose, while engineered E. coli produces 1.19 g L−1 h−1 with a yield of 0.82 mol mol−1 [14, 15]. The theoretical maximal yield of 2,3-BD from glucose is 1 mol per mol (0.5 g per g), and it was almost reached with pathogenic (Klebsiella spp.), and non-pathogenic producers (Bacillus spp.) (Additional file 1: Table S5 and references therein). Compared with these non-native producers, the best C. glutamicum 2,3-BD producer, ΔaceEΔpqoΔldhAΔmdh(pEKEx2-als,aldB, Ptuf butA), has a productivity close to the lower limit (10.9 nmol min−1 mg CDW−1 corresponding to 0.21 g L−1 h−1), and a good yield (0.66 mol 2,3-BD per mol glucose). Our work used cell suspensions at a relatively low OD600 (20–30, corresponding to about 5 g CDW L−1), but C. glutamicum can easily be grown to much higher cell density, allowing for higher 2,3-BD productivity during the production phase. For example, the utilization of a high density bioreactor (50 g CDW L−1), as in , would lead to one order of magnitude greater productivity (around 2 g L−1 h−1), which compares well with that of the non-pathogenic natural producer . Further increase in GCR of engineered C. glutamicum strains might be possible with a more fine manipulation of the oxygen supply conditions.
While this manuscript was in a late stage of preparation, a study was published by Yang et al.  with the same purpose as ours, albeit using different engineering strategies, host strains and production process. The 2,3-BD yield obtained was lower than that presented here (0.47 vs 0.66 mol per mol glucose), but a more extended comparison is hampered by the very different production processes used in the two studies.
By using a systematic approach C. glutamicum was successfully engineered for the production of 2,3-BD (Fig. 5). Organic acid production was strongly reduced or eliminated and adequate activities of the 2,3-BD biosynthetic pathway were achieved. By means of genetic engineering and manipulation of production conditions, productivity and yield were optimized. Characterization of production provided insight into metabolic features of producer strains, and indicated directions for further rounds of strain improvement. Future work should aim at increasing 2,3-BD yield by eliminating the side-products DHA and glycerol. By using the full potential of C. glutamicum, improvement of productivity and titer is also feasible. Additionally, we propose that the optimized construct, under adequate aeration conditions, can be used as a GRAS-platform for production of acetoin, another valuable chemical widespread in the food industry as flavor enhancer. Alternatively, straightforward developments, e.g., omission of the butA gene in the artificial operon and disruption of endogenous BDH, are expected to yield efficient acetoin producers.
Bacterial strains and growth conditions
Strains and plasmids used in this work are shown in Table 1. Cells were grown aerobically in the 2× TY medium described by Sambrook and Green . Medium was supplemented either with 0.5 % (wt/vol) glucose or with 1 % (wt/vol) potassium acetate. Plasmid-harbouring strains were selected using kanamycin (25 μg mL−1). Gene expression was induced by using 0.5 mM isopropyl β-d-1-thiogalactopyranoside (IPTG). Cultivations were performed at 30 °C with constant agitation at 160 rpm and were initiated by addition of a pre-culture to an optical density at 600 nm (OD600) of about 0.3. Growth was monitored by measuring the OD600. Specific growth rates (μ) were calculated through linear regression of the plots of ln(OD600) versus time during the exponential growth phase. For growth characterization, samples (1 mL) were taken periodically and pH was measured.
For the molecular biology procedures, E. coli DH5α was grown in test tubes containing 5 mL of 2× TY medium at 37 °C and 180 rpm. Plasmid selection was achieved using 50 μg kanamycin per mL.
Construction of strains and plasmids
All primers used are listed in Additional file 1: Table S2. To construct control strain C. glutamicum ∆ldhA, deletion of ldhA (cg3219) gene was performed according to , using the primer pairs described there. Deletion of the mdh (cg2613) gene in C. glutamicum ∆aceE∆pqo∆ldhA (aceE, cg2466; pqo, cg2891; ) was performed as described in . Chromosomal DNA of L. lactis MG1363, isolated according to , was used as template in PCR amplifications. In the first cloning step, the α-acetolactate synthase gene (als) was amplified from L. lactis chromosome using primer pair als-FW and als-RE and cloned into plasmid pEKEx2. In the second step, genes encoding the α-acetolactate decarboxylase (aldB) and 2,3-butanediol dehydrogenase (butA) of L. lactis were amplified using primers aldB-FW, aldB-RE, butA-FW and butA-RE, ligated, and subsequently inserted into pEKEx2-als, giving pEKEx2-als,aldB,butA. Alternatively, gene butA fused with 185 bp region upstream of tuf gene (Ptuf) was synthesized by NZYTech (Lisbon, Portugal). Plasmid pUC57 containing Ptuf-butA fusion was amplified in E. coli DH5α and restricted using BamHI and KpnI. The Ptuf-butA fragment was purified from agarose gel and ligated to aldB, after which joint DNA fragment was inserted into pEKEx2-als, yielding pEKEx2-als,aldB, Ptuf butA. Plasmids were obtained and maintained in E. coli DH5α. After verification of the correctness of the insert by sequencing (GATC, Konstanz, Germany), plasmids were isolated from E. coli and electroporated into competent C. glutamicum cells using the procedure described in  and . Then, plasmids were isolated from C. glutamicum in the following way: 5 mL of overnight culture was centrifuged for 1 min at 16,100×g and room temperature, to be re-suspended in 0.2 mL of solution A (50 mM glucose, 25 mM Tris–HCl, 10 mM EDTA, pH 8.0, freshly prepared). One μL of RNAse A (10 mg mL−1), and 15 mg mL−1 (final concentration) lysozyme were added, and the lysis was performed for 1.5 h at 55 °C. After the initial lysis step, isolation was continued with comercially available kits according to supplier instructions (Qiagen MiniPrep or Illustra Plasmid Mini Preparation Kit, GE Healthcare). Isolated plasmids were used as templates for PCR amplification of the inserted genes. Amplified region sequence was confirmed to be correct by sequencing (GATC, Konstanz, Germany).
Preparation of cell suspensions
Cells grown as described above were harvested 14 h after inoculation, centrifuged (3214×g, 10 min, 4 °C), and washed once with 0.9 % (wt/vol) NaCl. The resulting cell suspension was centrifuged (3214×g, 10 min, 4 °C) and the pellet was re-suspended in a minimal CGXII basal solution at pH 7.0, that contained per liter: 1 g KH2PO4, 1 g K2HPO4, 21 g MOPS (3-[N-morpholino] propanesulfonic acid), 0.25 g MgSO4·7 H2O, 10 mg CaCl2·2 H2O . Nitrogen sources (urea and (NH4)2SO4) were omitted, in order to minimize the biosynthesis of amino acids during the production phase.
Two-stage fermentations processes
C. glutamicum strains were grown and cell suspensions prepared as described above. For the second fermentation stage (production phase), 50 mL of cell suspension (OD600 of 15–20) were placed in an 80-mL fermenter (mini-fermenter), kept at 30 °C with a water bath and mixed with a magnetic stirrer at 200 rpm. Aeration was performed by sparging sterile air at a rate of 5, 10 or 20 mL min−1. The oxygen electrode (InPro® 6100/320/T/N, Mettler Toledo), was used to attempt monitoring dissolved oxygen during the production stage. The electrode was calibrated to 0 and 100 % after equilibration with pure argon and air, respectively. Glucose was provided to a final concentration of 2 % (wt/vol) and samples were collected over a period of 30 h. For the first round evaluation of the performance of the several constructs, 25 mL of concentrated cell suspension (OD600 of between 20 and 30) were placed in 50 mL closed falcon tubes kept at 30 °C in a rotary shaker (180 rpm). Glucose was provided to a final concentration of 2 % (wt/vol) and the fermentation was allowed to proceed for 48 h. Samples (1 mL) were centrifuged for 5 min at room temperature and 16,100×g; supernatants were then separated and kept at −20 °C until further analysis. End-products of metabolism were quantified by using 1H-NMR.
C. glutamicum strains were grown as described above and cell suspensions prepared in 50 mM PIPES at pH 7.0. Crude cell extracts were prepared by using glass beads (<106 μm) in a MiniBeadbeater-8 cell disrupter (Biospec Products) in 3 cycles of 1 min, with breaks of 3 min during which the extracts were kept on ice. After disruption, extracts were centrifuged at 16,100×g for 20 min at 4 °C. All enzyme activities were assayed at 30 °C in a Beckman Coulter DU 800 spectrophotometer in 50 mM PIPES (pH 7.0). One unit of enzyme activity corresponds to 1 μmol of substrate/product converted/formed per minute under the experimental conditions applied. The protein concentration was determined using Pierce BCA Protein Assay Kit (Thermo Scientific). Specific activity was expressed as units (μmol min−1) per milligram of protein [U (mg of protein)−1]. α-Acetolactate synthase activity was determined as described by . The reaction was stopped by the addition of 100 μL of 6 N H2SO4, and acetoin was quantified colorimetrically at 525 nm as described by Westerfeld . Butanediol dehydrogenases were assayed as described by Stormer , in a modified reaction mixture containing 50 mM buffer, 0.2 mM NADH and 2.5 mM racemic acetoin.
All 1H-NMR spectra were acquired on a Bruker AVANCE II + 400 MHz spectrometer (Bruker BioSpin GmbH) at 27 °C, using a BBO-F probe head. Pre-saturation of the residual water signal was applied. Acquisition parameters: flip angle of 90°; 32 K acquisition data points; repetition delay of 31.5 s. Formate was used as a concentration standard. The high reproducibility of the NMR measurements is illustrated in Additional file 1: Fig. S4 to justify the acquisition of a single spectrum for each biological replicate (Tables 3, 4).
Chemicals and reagents
For the molecular biology purposes, RNAse A and Pwo polymerase were purchased from Roche Life Science; lysozyme (Fluka) was purchased from Sigma-Aldrich, while all other enzymes were from New England Biolabs. Acetoin used in enzymatic assays was from Sigma-Aldrich. All other chemicals were commercially available reagent-grade (Sigma-Aldrich or Merck Sharp & Dohme).
DR was involved in designing the study, all stages of experimental work and writing the manuscript. ALC contributed to construction of producer strains and enzymatic activities measurements. SW was involved in strain construction. HS, BB, BJE, and ARN contributed to study design, supervision and manuscript preparation. All authors read and approved the final manuscript.
This work was supported by Fundação para a Ciência e a Tecnologia, Portugal (FCT), and FEDER, projects ERA-IB/BIO/0002/2008 and MOSTMICRO UID/CBQ/04612/2013. D.R. acknowledges FCT for the award of Ph.D. grant SFRH/BD/73265/2010. The NMR spectrometers are part of the National NMR Facility, supported by Fundação para a Ciência e a Tecnologia (RECI/BBB-BQB/0230/2012). We thank D. L. Turner for a critical reading of the manuscript, Nuno Borges for helpful advice, and Sara Rebelo for technical assistance.
The authors declare that they have no competing interests.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. 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.
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