- Open Access
Metabolic engineering of Bacillus subtilis for growth on overflow metabolites
© Kabisch et al.; licensee BioMed Central Ltd. 2013
- Received: 7 February 2013
- Accepted: 8 July 2013
- Published: 25 July 2013
The genome of the important industrial host Bacillus subtilis does not encode the glyoxylate shunt, which is necessary to utilize overflow metabolites, like acetate or acetoin, as carbon source. In this study, the operon encoding the isocitrate lyase (aceB) and malate synthase (aceA) from Bacillus licheniformis was transferred into the chromosome of B. subtilis. The resulting strain was examined in respect to growth characteristics and qualities as an expression host.
Our results show that the modified B. subtilis strain is able to grow on the C2 compound acetate. A combined transcript, protein and metabolite analysis indicated a functional expression of the native glyoxylate shunt of B. lichenifomis in B. subtilis. This metabolically engineered strain revealed better growth behavior and an improved activity of an acetoin-controlled expression system.
The glyoxylate shunt of B. licheniformis can be functionally transferred to B. subtilis. This novel strain offers improved properties for industrial applications, such as growth on additional carbon sources and a greater robustness towards excess glucose feeding.
- Bacillus subtilis
- Metabolic engineering
- Glyoxylate cycle
- Expression system
- Glycolic acid
The anaplerotic glyoxylate cycle is a variation of the tricarboxylic acid cycle (TCA cycle), which allows acetyl-CoA to be used to replenish carbon for anabolic processes . The isocitrate lyase of this shunt prevents a carbon loss by cleaving isocitrate into glyoxylate and succinate, thus avoiding the decarboxylation of isocitrate and 2-oxoglutarate. Glyoxylate and acetyl-CoA are joined to malate by the malate synthase, the second enzyme of the glyoxylate shunt, which allows for the regeneration of oxaloacetate that is henceforth available for anabolic activities via the TCA cycle or gluconeogenesis. From a bioprocessing viewpoint, this ability is especially interesting for bacteria that previously produced overflow metabolites. In terms of Bacillus subtilis such conditions include aerobic growth with excess glucose or anaerobic nitrate respiration [2, 3] and lead to the formation of acetate as well as acetoin and 2,3-butanediol. Industrial fermentation processes are usually so designed that overflow metabolism is avoided or at least limited. The overflow metabolism leads to metabolic shifts towards less efficient pathways and causes energy spilling reactions . Nevertheless the mixing of incoming, highly concentrated feed solutions is insufficient in industrial-scale bioreactors and always gives rise to zones of excess carbon source . For Escherichia coli it has been shown that the formation of overflow metabolites, especially acetate, hampers large scale fed-batch processes. Accumulated acetate has been observed to have adverse effects on target product formation and cell growth .
After depletion of the preferred carbon source (e.g. glucose), the excreted overflow metabolites are converted into metabolically utilizable acetyl-CoA . Since B. subtilis lacks the capability to conduct the glyoxylate cycle, it can only make use of the energy provided by the overflow metabolites in the form of reduction equivalents, which are generated during the TCA cycle. In this study the transfer of the glyoxylate shunt - operon from its close relative Bacillus licheniformis was investigated in B. subtilis. It is shown that the functional expression of this operon enables B. subtilis to utilize the overflow metabolite acetate as a carbon source and resulted in a more robust growth behavior with excess glucose and an increased production of a recombinant reporter enzyme.
First attempts to construct plasmids containing the complete glyoxylate operon of B. licheniformis failed with E. coli as subcloning host. Transformation of the ligation reaction using E. coli as a shuttle host resulted in plasmids containing different fragments of the genes, but never the complete operon, making it likely that ORFs of the glyoxylate operon are expressed in E. coli and interfere with its metabolism. Therefore, we constructed the plasmids in such a manner that one plasmid contained only the aceB and the aceA genes without a promoter and another plasmid contained the native aceBA-operon specific promoter and the above mentioned hypothetical protein (Figure 1B). Both plasmids could be propagated in E. coli and the transformation of B. subtilis in a two-step-procedure worked well, yielding B. subtilis ACE which contains the native glyoxylate operon of B. licheniformis in its chromosomal amyE locus.
Relatively little is known about the regulation of the glyoxylate cycle in Gram-positive bacteria. Results of this study indicate a control of the aceBA-operon of B. licheniformis in B. subtilis at the transcriptional level. A transcriptional regulation of the glyoxylate shunt has also been shown for the Gram-positive bacterium Corynebacterium glutamicum, where the expression of the malate synthase and isocitrate lyase is positively controlled by the LuxR-type transcriptional regulator RamA in the presence of acetate . Voigt et al. detected a strong induction of the AceB expression in B. licheniformis at the transcriptional and translational level as soon as the preferred carbon and energy source glucose is exhausted . Schroeter et al.  could determine an induction of the glyoxylate shunt during peroxide stress experiments, which was attributed to an irreversible oxidation of the isocitrate dehydrogenase (ICDH). However, it is also shown in our study that the region encoding the hypothetical protein (BL02643) in front of aceBA is essential for a functional transfer of the glyoxylate shunt to B. subtilis. Strain constructs missing this putative regulatory region of the operon fail to grow on acetate (data not shown). It can be concluded that this small protein plays an essential role in the regulation of the glyoxylate cycle activity.
The incorporation of the glyoxylate shunt - encoding operon led to growth of B. subtilis ACE on the overflow metabolite acetate and to a lesser degree on acetoin. A diauxic growth with a preferred utilization of glycerol over acetate can be derived from the metabolite analyses (Figure 4). However, the current version of the glyoxylate cycle - positive strain B. subtilis ACE failed to reach the same maximal optical density as B. licheniformis (data not shown). A possible reason for its earlier growth arrest might be the accumulation of glycolic acid (see Figure 4). This small alpha-hydroxy acid has been described as a potent inhibitor of the isocitrate lyase of Pseudomonas indigofera and could disable B. subtilis ACE to continue utilizing acetate as a replenishing carbon source through its glyoxylate cycle. Glycolic acid is also formed in B. licheniformis, but to a much smaller extent (data not shown). B. licheniformis DSM13 possesses a putative glyoxylate reductase (ORF BL02138) which exhibits a 70% identity to a similar enzyme (gyaR) of Bacillus pumilus ATCC 7061. This putative glyoxylate reductase (ORF BL02138) could catalyze the reduction of glyoxylate to glycolic acid and could thus lead to a reduced accumulation of glycolic acid in B. licheniformis.
The accumulation of 2.3-butanediol in B. subtilis during the exponential and stationary phase is likely due to the activity of the acetoin reductase/2.3-butanediol dehydrogenase (bdhA) . The remaining acetoin could block the reverse reaction that would transform the 2.3-butanediol back to acetoin. It has been reported that the presence of acetic acid leads to an increased production of 2.3-butanediol by B. subtilis. In contrast, B. licheniformis is able to utilize acetoin but also 2.3-butanediol entirely (data not shown), which might also have contributed to an increase of biomass. This is most probably also supported by the butanediol/acetoin reductase encoded by the budC (BL01177) gene of B. licheniformis, which catalyzes the irreversible reduction of 2.3-butanediol to acetoin . Interestingly, the subspecies B. subtilis subsp. spizizenii, which is of a different lineage than the used B. subtilis strain 6051HGW , encodes the same potential for the 2.3-butanediol utilization as B. licheniformis, highlighting both as potential donors of the butanediol/acetoin reductase for a further optimization of B. subtilis ACE.
The simulated EnBase fed-batch cultivation indicated an advantage of the glyoxylate shunt - active strain B. subtilis ACE in comparison to the WT under high glucose concentration conditions. Induction of a significant overflow metabolism by addition of excess glucose presumably resulted in the growth arrest of the WT, while the activity of the glyoxylate shunt enabled B. subtilis ACE to exploit too high levels of these metabolites and to reach thus elevated cell densities.
This study indicates that the previously described acoA-expression system  displays an improved performance in the glyoxylate cycle - positive strain B. subtilis ACE. The promoter of the acoABCL-operon is repressed by PTS–sugars , but as demonstrated in this study also by the non-PTS carbon source glycerol. The cheap C-source glycerol in combination with acetate therefore offers an interesting alternative for the control of the acoA-based B. subtilis expression system. Another possible application of B. subtilis ACE may be an auto-inducing system that depends on phosphate limitation. As described by Dauner et al., B. subtilis produces large quantities of acetate during chemostat experiments with high glucose and low phosphate levels. The ability of B. subtilis ACE to produce higher recombinant target protein levels, while growing on acetate, would therefore be a suitable alternative possibility for the application of the acoA-expression system.
The aceBA operon of B. licheniformis is a self-contained metabolic entity that can be functionally transferred to B. subtilis. The obtained strain is able to grow on acetate as carbon source which results in an increased biomass formation and an improved production of a recombinant model protein. In addition, the glyoxylate cycle-positive B. subtilis mutant cells feature greater robustness towards excess glucose cultivations.
Construction of plasmids, strains, and genome analysis
Oligonucleotide primers used in this study
Sequence 5’ → 3’
Forward primer for aceBA operon
Reverse primer for aceBA operon
Forward primer for integration of native promoter
Reverse primer for integration of native promoter
Forward primer for Ery R cassette
Forward primer for Ery R cassette
Forward primer for mRNA-standard of aceB
Reverse primer for mRNA-standard of aceB
Reverse primer for mRNA-standard of aceB with T7-promoter
Strains and plasmids used in this study
B. subtilis 6051HGW
B. licheniformis MW3
B. subtilis ACE
B. subtilis ACEProm1
B. subtilis ΔamyE
B. subtilis acoAamyE
ΔamyE::Ery R ΔsacA::acoAamyESSS
B. subtilis ACEamyE
E. coli DH10B
F-mcrA,(mrr-hsdRMS-mcrBC)’80lacZ, M15, lacX74, recA1 araD139, (ara leu) 7697
Integration of genes into the amyE locus with NeoR
aceBA chromosomal integration into the amyE locus without promoter
Source of ermB gene for erythromycin resistance
Integration of genes into the amyE locus with EryR
Integrating of the native aceBA promoter and the gene encoding the hypothetical protein
Integration of genes into the sacA-locus
J. Kumpfmüller (unpublished results)
Source of the P acoA -amyE construct
Integration of the amyE gene under P acoA control into the sacA-locus
The plasmid pACEBA was constructed by amplifying the aceBA-operon without its predicted promoter region and the hypothetical protein. The PCR product and the pBGAB  plasmid were cut with XbaI and BamHI and ligated using T4-ligase. To integrate the native promoter and the hypothetical protein in front of the aceBA-operon, the pBGAG plasmid was cut with SmaI and NotI and an erythromycin cassette from pMTL500  was inserted yielding the plasmid pAMYSSE. Hereafter, this plasmid was cut with NarI and EcoRI and the PCR product resulting from the Prom1-primer pair was integrated via a modified sequence and ligation-independent cloning method . Electroporation of the plasmids into E. coli was performed as previously described . All utilized enzymes were purchased from New England Biolabs (Frankfurt a. M., Germany), oligonucleotides were synthesized by Life Technologies (Darmstadt, Germany).
To obtain an aceBA-encoding strain, B. subtilis 60-51HGW was transformed via natural competence  using the linearized plasmid pACEBA. The clones were selected on neomycin and the positive mutants were designated as B. subtilis ACE-P. To functionalize the operon, pProm1 was transformed in the same manner into B. subtilis ACE-P with erythromycin selection resulting in B. subtilis ACE. To examine the expression of a reporter enzyme, B. subtilis ACE and B. subtilis 6051HGW were transformed with pSacAmyE yielding a wild type (B. subtilis WTamyE) and a glyoxylate cycle - positive mutant (B. subtilis ACEamyE) that express and secrete an alpha-amylase under control of the acoA-promoter . pSacAmyE was constructed by cutting pJK168 and pMJS2  with XbaI and ligating the acoA-amyE fragment from pMJS2 into the sacA landing pads of pJK168. To ensure comparable alpha-amylase measurements, the native alpha-amylase of B. subtilis was disrupted by the integration of the aceBA- operon (B. subtilis ACEamyE) and an erythromycin cassette of plasmid pAMYSSE (B. subtilis WTamyE) into the amyE-locus. All plasmid constructs and chromosomal integrations were verified by sequencing.
The publicly available genome sequence of B. licheniformis was annotated in 2004 . Since then, a large amount of novel sequences and annotations have been published, which implicates the necessity to update previous functional assignments for organisms of interest. Accordingly, we reannotated the genome sequence of B. licheniformis DSM13 in the same manner as described for B. subtilis 6051HGW . In short, the GenBank file of B. licheniformis DSM13 [GenBank:AE017333] was imported into the GenDB 2.2  pipeline and the resulting database was used to analyze the ORFs with JCoast .
Cultivations were carried out at 37°C and 250 rpm shaking in Erlenmeyer flasks with a maximum culture volume of one fifth of the flasks volume. Pre-cultures were inoculated from a cryo-stock and grown in LB medium for 5 h and then transferred into the appropriate medium for overnight cultures. Main cultures were inoculated from exponentially growing overnight cultures. The composition of the mineral salt medium (MSM) and its trace element solution has been described previously . The MSM was supplemented with 0.08% glycerol, 0.5% acetate, 0.2% acetoin, and 2 mM MgSO4 if not indicated otherwise.
In order to test fed-batch like conditions, we cultivated the glyoxylate cycle - positive mutant and the WT strain with 3 ml EnBase Flo Liquid (# EBLM500, BioSilta Oy, Oulu, Finland) medium in 24-deep-well plates. The EnBase system is based on the slow release of glucose from a polymer through the action of an enzyme, thus acting like a substrate feeding pump . The native amylase of B. subtilis (amyE) has been reported to interfere with this method (personal communication P. Neubauer). Therefore, B. subtilis amylase knock-out strains (Table 2) were used in all EnBase cultivations. Beside the control culture without external glucose addition, cultures supplemented with 0.2% and 0.4% glucose were investigated to simulate high glucose conditions and to stimulate acetate formation. 1.5 U of the EnBase-specific hydrolase (BioSilta Oy, Oulu, Finland) was used in all experiments. Plates were shaken at 300 rpm with an amplitude of 25 mm. Sample volume was 10 μl, with which the OD at 500 nm was determined in a 1:10 dilution in a Tecan infinite M200 plate reader (Männerdorf, CH).
RNA samples were taken and prepared as previously described . An additional treatment with RNAse-free DNAse (#79254, Qiagen, Hilden, Germany) was performed followed by a purification with the RNA Clean-Up and Concentration Kit (#23600) from Norgen Biotek (Thorold, Canada).
The aceB-mRNA-standard was created with the primers aceB-for and aceB-rev-T7 (Table 1) using the DIG RNA Labeling Kit (SP6/T7) from Roche (Mannheim, Germany) and substituting the DIG-labeled nucleotides with unlabeled NTPs (Fermentas UAB, Vilnius, Lithuania).
The real-time RT-PCR analysis was performed as described by Hoi et al. . The RNA samples were prepared as recommended by the supplier of the LightCycler® RNA Master SYBR Green I (#03064760001, Roche). The RT-PCR reaction was prepared with the primers aceB-for and aceB-rev (Table 1) and analyzed applying the Roche LightCycler as suggested by the manufacturer with an annealing temperature of 56°C.
The supernatant required for the alpha-amylase reporter enzyme assay was obtained by centrifugation of 2 ml culture at 10000 x g for 5 min at 4°C. The resulting supernatant was transferred to a new tube and stored at -20°C until further processing. The amylase activity was determined by use of the Ceralpha Assay (Megazymes, Wicklow, Ireland). To stay within the linear range, 1:200 dilutions in the suggested buffer were prepared. Measurements were done with a Tecan infinite M200 plate reader.
For the cytosolic proteome analysis, 8 ml of cells were harvested by centrifugation and washed twice with TE-buffer (10 mM Tris-Cl, pH 7.5, 1 mM EDTA) and finally resuspended in 1 ml TE with 2 mM PMSF (Carl Roth, Karlsruhe, Germany). Samples were transferred to cryotubes (Sarstedt, Nümbrecht, Germany) filled with 0.25 ml glass beads (Sartorius AG, Göttingen, Germany) and the cells were disrupted by bead-beating for 30 seconds at 6.5 m/s. After cooling for 5 min on ice, this procedure was repeated twice. Cell debris was removed by 30 min centrifugation at 17000 x g. The supernatant was stored at -20°C. 5 μg of protein mixture were separated by SDS-PAGE  and stained with silver-blue Coomassie .
The bands were excised using a sterile scalpel and transferred into 96 well micro titer plates (Greiner bio one, Frickenhausen, Germany). The tryptic digest with subsequent spotting on a MALDI-target was carried out automatically with the Ettan Spot Handling Workstation (Amersham Biosciences, Uppsala, Sweden). The gel pieces were washed twice with 100 μl of a solution of 50% CH3OH and 0% 50 mM NH4HCO3 for 30 min and once with 100 μl 75% CH3CN for 10 min. After drying at 37°C for 17 min 10 μl trypsin solution containing 4 μg/ml trypsin (Promega, Madison, WI, USA) was added and incubated at 37°C for 120 min. For extraction gel pieces were covered with 60 μl 0.1% TFA in 50% CH3CN and incubated for 30 min at 40°C. The peptide-containing supernatant was transferred into a new microtiter plate and the extraction was repeated with 40 μl of the same solution. The supernatants were completely dried at 40°C for 220 min. The dry residue was resuspended in 0.9 μl α-cyano-4-hydroxy-cinnamic acid matrix (3.3 mg/ml in 50%/49.5%/0.5% (v/v/v) CH3CN/H2O/TFA) and 0.7 μl of this solution was deposited on the MALDI target plate. The samples were allowed to dry on the target 10 to 15 min before measurement by MALDI-TOF mass spectrometry.
The MALDI-TOF measurement was carried out on the AB SCIEX TOF/TOF™ 5800 Analyzer (ABSciex /MDS Analytical Technologies, Darmstadt, Germany). This instrument is designed for high throughput measurement, being automatically able to measure the samples, calibrate the spectra and analyze the data using the TOF/TOF™ Series Explorer™ SoftwareV4.1.0. The spectra were recorded in a mass range from 900 to 3700 Da with a focus mass of 1700 Da. For one main spectrum 25 sub-spectra with 100 shots per sub-spectrum were accumulated using a random search pattern. If the autolytical fragment of trypsin with the mono-isotopic (M + H) + m/z at 2211.104 reached a signal to noise ratio (S/N) of at least 40, an internal calibration was automatically performed as one-point-calibration using this peak. The standard mass deviation was less than 0.15 Da. If the automatic mode failed (in less than 1%), the calibration was carried out manually. The five most intense peaks from the TOF-spectra were selected for MS/MS analysis. For one main spectrum 20 sub-spectra with 125 shots per sub-spectrum were accumulated using a random search pattern. The internal calibration was automatically performed as one-point-calibration with the mono-isotopic arginine (M + H) + m/z at 175,119 or Lysine (M + H) + m/z at 147,107 reached a signal to noise ratio (S/N) of at least 5. The peak lists were created by using GPS Explorer™ Software Version 3.6 (build 332) with the following settings for TOF-MS: mass range, 900–3700 Da; peak density, 20 peaks per 200 Da; minimum S/N ratio of 15 and maximal 65 peaks per spot. The TOF-TOF-MS settings were a mass range from 60 to Precursor - 20 Da; a peak density of 50 peaks per 200 Da and maximal 65 peaks per precursor. The peak list was created for an S/N ratio of 10. All peak lists were analysed using Mascot search engine version 2.4.0 (Matrix Science Ltd, London, UK) with a specific user sequence database and specific B. subtilis and B. licheniformis databases.
1H-NMR for extracellular metabolite analysis
2 ml cell culture was rapidly sterile filtered into a 2 ml tube and stored at -20°C. 400 μl of the extracellular sample was buffered to pH 7.0 by addition of 200 μl of a sodium hydrogen phosphate buffer (0.2 mM [pH 7.0], including 1 mM TSP)) made up with 50% D2O to provide a nuclear magnetic resonance (NMR)-lock signal. The samples were measured using 1H-NMR (600.27 MHz) at a nominal temperature of 310 K (Bruker AVANCE-II 600 NMR spectrometer, Bruker Biospin GmbH, Rheinstetten, Germany) as described previously . AMIX 3.9 was used for data processing and analysis.
Graphs were created using R  and, where applicable, with the ggplot2 package . Graphs for metabolites were created with VANTED V2.1.3 . Genome analysis was done with Geneious version 5.6.2 created by Biomatters (Auckland, NZ) available from http://www.geneious.com. Free Gibbs-Energy (-∆G) of mRNA structures was determined with UNAfold .
This study was financially supported by the German Federal Ministry of Education and Research (BMBF reference 0315400A/B) in the frame of the BIOKATALYSE2021 network and the BACELL-SysMo project (reference 031397A). We thank Jana Matulla and Daniel Götze for their excellent technical support and Stephanie Markert for critical reading of the manuscript.
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