A proteomic and transcriptional view of acidogenic and solventogenic steady-state cells of Clostridium acetobutylicum in a chemostat culture

Abstract

The complex changes in the life cycle of Clostridium acetobutylicum, a promising biofuel producer, are not well understood. During exponential growth, sugars are fermented to acetate and butyrate, and in the transition phase, the metabolism switches to the production of the solvents acetone and butanol accompanied by the initiation of endospore formation. Using phosphate-limited chemostat cultures at pH 5.7, C. acetobutylicum was kept at a steady state of acidogenic metabolism, whereas at pH 4.5, the cells showed stable solvent production without sporulation. Novel proteome reference maps of cytosolic proteins from both acidogenesis and solventogenesis with a high degree of reproducibility were generated. Yielding a 21% coverage, 15 protein spots were specifically assigned to the acidogenic phase, and 29 protein spots exhibited a significantly higher abundance in the solventogenic phase. Besides well-known metabolic proteins, unexpected proteins were also identified. Among these, the two proteins CAP0036 and CAP0037 of unknown function were found as major striking indicator proteins in acidogenic cells. Proteome data were confirmed by genome-wide DNA microarray analyses of the identical cultures. Thus, a first systematic study of acidogenic and solventogenic chemostat cultures is presented, and similarities as well as differences to previous studies of batch cultures are discussed.

Electronic supplementary material

The online version of this article (doi:10.1007/s00253-010-2741-x) contains supplementary material, which is available to authorized users.

Introduction

The obligate anaerobe Clostridium acetobutylicum is well known for its acetone–butanol (AB) fermentation (Dürre 2008; Jones 2001; Jones and Woods 1986; Lee et al. 2008). Transition from exponential to stationary growth typically comprises a metabolic change from the formation of acetate and butyrate towards the formation of acetone and butanol as the dominant fermentation products. Due to its past importance for the industrial production of the bulk chemicals acetone and butanol (Jones 2001; Jones and Woods 1986) and its potential for future solvent production, e.g., especially with respect to n-butanol as promising bio-based liquid fuel with several advantages over ethanol (Dürre 2007; Ni and Sun 2009), much research has focused on the regulation of the metabolic “shift”. Since the genome sequence of C. acetobutylicum was published (Nölling et al. 2001), transcriptomic and proteomic studies were included (Alsaker and Papoutsakis 2005; Jones et al. 2008; Sullivan and Bennett 2006; Tomas et al. 2003). Nevertheless, the regulation of solvent formation remains largely unknown yet. Although much valuable information was provided, all these studies generally exhibited poor reproducibility as a major drawback because all experimental data resulted from simple batch fermentations. As a prerequisite for further comparative analyses, defined growth conditions without constantly changing environmental conditions are required. Continuous cultivation constitutes a preferred fermentation method to accomplish standardized conditions with a maximum degree of reproducibility because cells are kept in a steady state with constant endogenous as well as exogenous parameters, such as growth rate, substrate, and product concentrations.

Almost 30 years ago, chemostat cultivation of C. acetobutylicum was performed to analyze various parameters affecting butanol production. Using a synthetic medium and phosphate limitation, C. acetobutylicum could be kept in a steady state of acidogenesis when the pH was >5 and in a steady state of solventogenesis at pH 4.3 for at least several months (Bahl et al. 1982a, b). Although this process was not considered to be competitive with industrial butanol production in the batch or fed-batch mode (Jones et al. 1982), chemostat cultures are valuable scientific applications in analyzing specific parameters with limited or ideally without any perturbations.

Systematic “omic” analyses of chemostat cells are still at their beginning. The aim of this study was to comprehensively compare C. acetobutylicum acidogenic and solventogenic steady-state cells to provide new insights into the metabolic changes. Stable growth rates and constant exogenous parameters during the chemostat fermentation process enabled homogeneity of bacterial cells, and the pH as single parameter was changed to switch from acidogenesis to solventogenesis. Thus, a “master” fermentation was established and used for detailed analyses of the proteome and transcriptome of the identical culture of steady-state cells growing at pH 5.7 and pH 4.5, respectively.

Material and methods

Organism and growth conditions

C. acetobutylicum ATCC824 (COSMIC strain) was grown under anaerobic conditions at 37°C according to a standard operation procedure developed for the COSMIC consortium (http://www.sysmo.net). Precultures starting from spore stocks were prepared as previously described (Fischer et al. 2006). The phosphate-limited chemostat experiments (n = 2) with 0.5 mM KH₂PO₄ and 4% (wt/vol) glucose in the supplying medium (Fiedler et al. 2008) were performed in a BiostatB 1.5-l fermenter system (BBI, Melsungen, Germany) at 37°C. The dilution rate (respective generation time) was D = 0.075 h⁻¹. After inoculation, cell growth caused a natural decrease of the pH. At pH 5.7, pH control was turned on and pH was kept constant by automatic addition of 2 M KOH until stable acidogenic steady state was reached and first sampling occurred. Then the pH control was temporarily turned off to induce solvent formation and was started again at pH 4.5, keeping the cells in stable solventogenic steady state when the second sampling took place (for further details, refer to “Results” section).

OD, phosphate concentration, and fermentation products

The measurement of the optical density at 600 nm (OD₆₀₀), phosphate concentration, and the analysis of the fermentation products were accomplished as described elsewhere (Fischer et al. 2006).

Isolation of total RNA, microarray experiments, and Northern blot analysis

The isolation of total RNA and DNase treatment was performed as previously described (Fischer et al. 2006). The integrity of the RNA samples was verified by gel electrophoresis. RNA concentrations were determined by their specific absorptions at A₂₆₀ nm. DNA-free RNA aliquots were transcribed into cDNA and cy3- or cy5-labeled, respectively. Microarray experiments using a DNA chip containing 3,840 spotted oligonucleotides of protein coding genes of C. acetobutylicum were performed as published recently (Hillmann et al. 2009). Microarray experiments were performed twice (n = 2), and duplicate arrays were hybridized with reverse-labeled samples (dye-flip: pH 5.7-Cy3/pH 4.5-Cy5 and pH 5.7-Cy5/pH 4.5-Cy3). Full lists of transcribed genes, functional information, and regulation are available in supplementary data SD5 and SD6. Microarray design and data are also available from the ArrayExpress database under accession no. E-MEXP-2503 (http://www.ebi.ac.uk/microarray-as/aer/entry).

Probes for the Northern hybridization were PCR-generated using standard protocols with Pwo polymerase (Peqlab, Biotechnology, Erlangen, Germany) and chromosomal DNA of C. acetobutylicum as template. Amplification of gene specific probes (cap0037 542 bp, cap0036 881 bp) based on the primers Cap0037_fw (5′-GAACAAGAGATGCTGTATTTTC-3′) and Cap0037_rev (5′-ACTTCTTGAGATAACTCATATTTC-3′) and Cap0036_fw (5′-TGTTTTATCATAGAAAGCCTTTTG-3′) and Cap0036_rev (5′-GAAAATACAGCATCTCTTGTTC-3′). The 16S rRNA probe (1,510 bp) amplified with the forward primer (Eub1, 5′-GAGTTTGATCCTGGCTCAG-3′) and the reverse primer (Eub2, 5′-AGAAAGGAGGTGATCCAGCC-3′) served as an internal control to ensure integrity and amount equity of the total RNA used. Labeling with digoxigenin (DIG) and Northern blot hybridization at 42°C (overnight) were performed according to the directions of the manufacturer (DIG DNA labeling and detection kit; Roche Diagnostic, Mannheim, Germany). Detection of chemiluminescence was performed as described previously (Fischer et al. 2006).

Two-dimensional gel electrophoresis

The soluble intracellular protein fractions of C. acetobutylicum cells were illustrated by two-dimensional polyacrylamide gel electrophoresis as described in detail by Schwarz et al. (2007). Proteins were visualized by colloidal Coomassie staining, and gels were documented by scanning (UMAX 2100, Biostep GmbH, Jahnsdorf, Germany). Gel images were transferred to Delta 2D software (version 3.5) for detailed analysis. All detected protein spots were identified by MALDI-TOF MS/MS.

MALDI-TOF MS/MS

Mass spectrometry was performed in a Proteomics Analyzer 4800 (Applied Biosystems, Foster City, USA) as published by Voigt et al. (2006), except that the signal to noise ratio for the TOF-TOF measurements was raised to 10. Proteins were identified using the Mascot search engine with a C. acetobutylicum databank (Matrix Science, London, UK; Voigt et al. 2006).

Results

Master fermentation

Cells of chemostat cultures are strongly recommended for “omic” analyses in contrast to batch cultures because exponentially growing cells can be kept at specifically defined physiological conditions without any transient changes in the environment. Thus, chemostat cultivation optimally allows analyses of the effects of single external parameter changes. In this study, acidogenic or solventogenic metabolism of C. acetobutylicum chemostat cells was directed exclusively by the external pH values of pH 5.7 or pH 4.5, respectively. Under both steady-state conditions, only vegetative cells and no other differentiated cell forms like clostridial stages, prespores containing cells, or mature spores were detected.

A typical continuous chemostat culture referred to as “master” fermentation is described in Fig. 1. The time course of a master fermentation was subdivided into four parts (I–IV). Phase I reflects the time period after starting the medium pump, the transition of batch growth to continuous pH-controlled growth at pH 5.7. Typically, acidogenic cells of phase I exhibited highest cell densities of up to OD 10 and consequently the highest butyrate and acetate concentrations measured throughout the master fermentation. After approximately 3 days (t = 65–80 h), stable cell densities (OD 5 ± 0.5) and fermentation products (acetate ~35 mM, butyrate ~60 mM) indicated the beginning of phase II, balanced steady-state growth at pH 5.7. To ensure the steady state, sampling took place at least 24 h later (usually 1 to 2 days later, respective 4 to 5 days (t = 96–120 h) after starting continuous growth). Thereafter, the pH control was turned off, initializing phase III. Promptly, the external pH decreased. This exclusive external signal induced reorganization of the metabolism of C. acetobutylicum from acidogenesis to solventogenesis, and at pH 4.5 (~15–20 h later), the pH control was turned on again. Lowering of the pH was typically accompanied by a transient drop of the cell densities documented by minimal OD values of about 3. Steady-state growth at pH 4.5 was usually reached within 48 h after the drop of the pH, the beginning of phase IV. At least 3 days later (around 10 days or 240 h after starting the continuous cultivation), the second sets of samples were drawn for the analyses of solventogenic cells.

Fig. 1.

“Master” fermentation of C. acetobutylicum. Monitored 240 h after starting the medium supply at t₀. a shows pH (filled upright triangles) and optical density (empty squares); b illustrates the pH (filled upright triangles) and the fermentation products butyrate (filled squares), acetate (filled inverse triangles), butanol (empty upright triangles), acetone (empty circles), and ethanol (filled circles). Roman numbers highlight the four different phases, I: starting of continuous culture; II: establishing of steady-state growth at pH 5.7; III: switch of pH from 5.7 to 4.5; IV: establishing of steady-state growth at pH 4.5 of the fermentation. Arrows indicated sampling points for proteome and transcriptome analyses at the end of phase II and phase IV

Proteome analysis

Representative 2-D gels of acidogenic steady-state and solventogenic steady-state cells growing at pH 5.7 or pH 4.5, respectively, are shown in Figs. 2 and 3. The complete novel proteome reference maps are presented in supplementary data file SD1 (Figs. S1 and S2) in combination with files SD2 and SD3. The cytoplasmic protein extracts revealed a coverage of more than 21% of proteins with calculated isoelectric points between pH 4 and pH 7 and molecular weights between 10 and 200 kDa (Hiller et al. 2006). Protein extracts of acidogenic cells yielded 357 spots with 178 identified different proteins whereas in solventogenic cells 205 different proteins were represented in 415 spots.

Fig. 2.

Representative colloidal Coomassie-stained 2-D gel of cytosolic proteins from cells grown at pH 5.7. The numbers highlight protein spots with higher abundance in acidogenic cells; respective proteins are listed in Table 1

Fig. 3.

Representative colloidal Coomassie-stained 2-D gel of cytosolic proteins from cells grown at pH 4.5. The numbers highlight protein spots with higher abundance in solventogenic cells; respective proteins are listed in Table 2

For the elucidation of characteristic proteins of cells grown at pH 5.7 and at pH 4.5, respectively, the data were screened for proteins with enhanced appearance (supplementary data files SD1 with Figs. S1 and S2, SD2, and SD3). Significance was defined as an at least twofold increase in spot intensity in comparison to the spots in the gels of the compared pH. Accordingly, 2-D gels of acidogenic cells at pH 5.7 revealed 15 enhanced spots as highlighted in Fig. 2 and further described in Table 1.

Table 1.

Proteins with increased (≥2.0) abundance in the acidogenesis at pH 5.7

^aProteins of spots with more than one polypeptide are listed in their identification order

^bNames based on Nölling et al. (2001)

^cCorresponding spot numbers in Fig. 2

^dIf more than one protein spot was detected, the average of all protein spots is shown (SD 4)

^eThe sign for nonterminating (∞) indicates that the protein was not detectable at pH 4.5

Most noticeable were the proteins CAP0037 and CAP0036. Their genes are located on the megaplasmid pSOL1 (Cornillot et al. 1997), and both were annotated as uncharacterized gene products with unknown functions (Nölling et al. 2001). Both proteins were present in multiple spots, up to five in the case of CAP0037 and at least up to four in the case of CAP0036 (Fig. 2, Table 1). None of these spots were detectable in 2-D gels of solventogenic cells grown at pH 4.5. Their horizontal spot distributions indicated three different isoelectric points for each protein due to different protein charges. Additionally, CAP0037 revealed two different apparent molecular masses of 22 and 25 kDa, indicating posttranslational modifications, such as phosphorylation, acetylation, glycosylation, or methylation, which have been reported to occur in C. acetobutylicum (Balodimos et al. 1990; Lyristis et al. 2000; Sullivan and Bennett 2006) and other prokaryotic organisms (Rosen and Ron 2002; Rosen et al. 2004).

Another interesting spot with increased abundance (~2.1-fold) at pH 5.7 revealed electron transfer flavoprotein beta-subunit (EtfB, CAC2710). The etfB gene is part of the etfA–etfB–bcd–crt operon (CAC2709–CAC2712) whose mRNA transcript was also significantly elevated at pH 5.7 (~3.0–3.5-fold, Table 3 and supplementary data file SD1, Table S2). EtfA, EtfB, and Bcd showed multiple spots in the 2-D gels (supplementary data file SD1, Table S1), but only EtfB revealed a significantly higher abundance.

Table 3.

Genes with a significant induction at the transcript level at pH 5.7

ORF#	Gene	Protein functiona	1. array	2. array	3. array	4. array	Average fold reg.	SD	COGb
CAC0029		Distantly related to cell wall-associated hydrolase, similar to yycO B. subtilis	2.1	1.5	7.5	3.2	3.6	2.7	S
CAC0149		Hypothetical protein	5.9	5.2	14.5	10.1	8.9	4.3	–
CAC0164		ABC transporter, ATP binding protein	2.4	2.0	9.4	2.9	4.2	3.5	V
CAC0231		Transcriptional regulator of sugar metabolism	3.5	2.7	12.1	3.7	5.5	4.4	K,G
CAC0232	fruB	1-phosphofructokinase	2.2	1.9	11.8	2.9	4.7	4.8	G
CAC0233		PTS system, IIA component	2.5	2.0	18.2	2.3	6.2	8.0	G,T
CAC0234		PTS system, fructoso-specific IIBC component	2.2	2.1	8.1	3.0	3.9	2.9	G
CAC0360		Transcriptional regulator	3.1	2.6	6.5	5.6	4.5	1.9	K
CAC0407		PP2C phosphatase family	2.7	2.1	4.6	3.5	3.2	1.1	T
CAC0409		Hypothetical protein	2.1	1.9	5.7	3.2	3.2	1.8	–
CAC0410		Hypothetical protein	2.0	1.8	5.6	2.6	3.0	1.8	S
CAC0411		Hypothetical protein	2.8	2.3	7.3	5.3	4.4	2.3	S
CAC0412		TPR-repeat-containing protein	2.0	1.7	5.5	3.9	3.3	1.8	R
CAC0427		Glycerol-3-phosphate ABC transporter, permease component	3.1	3.1	5.7	2.9	3.7	1.3	G
CAC0428		Sugar permease	4.2	2.7	11.2	3.5	5.4	3.9	G
CAC0429		Glycerol-3-phosphate ABC transporter, periplasmic component	4.6	3.3	9.2	5.7	5.7	2.5	G
CAC0430		Glycerophosphoryl diester phosphodiesterase	2.2	3.5	7.1	6.8	4.9	2.4	C
CAC0742		Phosphatase domain-containing protein	2.2	1.8	6.3	3.1	3.3	2.0	I
CAC0946		ComE-like protein	2.8	2.4	4.6	3.9	3.4	1.0	R
CAC1081		Hypothetical protein	2.1	2.1	13.0	5.6	5.7	5.1	S
CAC1230		Hypothetical protein	2.6	2.6	6.9	2.3	3.6	2.2	–
CAC1231		Predicted dehydrogenase	2.0	1.7	7.1	3.8	3.6	2.5	R
CAC1547	trxA	Thioredoxin	4.1	3.4	8.3	6.8	5.6	2.3	O
CAC1548	trxB	Thioredoxin reductase	3.3	3.6	6.9	5.2	4.8	1.7	O
CAC1549	bsaA	Glutathione peroxidase	2.8	2.7	8.3	3.2	4.2	2.7	O
CAC1583		Predicted P-loop ATPase	2.4	2.2	3.5	5.3	3.3	1.4	E
CAC1702		Hypothetical protein	3.2	3.0	4.9	5.0	4.0	1.1	–
CAC1703		Methyl-accepting chemotaxis protein (fragment)	2.4	2.5	5.2	4.4	3.6	1.4	N,T
CAC1704		Hypothetical protein	2.8	2.8	4.9	5.0	3.9	1.2	–
CAC2252		Alpha-glucosidase	1.9	2.3	7.1	5.2	4.1	2.5	G
CAC2342		Predicted membrane protein	4.1	4.3	2.1	3.4	3.5	1.0	R
CAC2365	sspA	Small acid-soluble spore protein	13.1	13.9	6.1	–	11.0	4.3	–
CAC2438		Predicted phosphatase	5.3	4.7	3.4	4.8	4.5	0.8	–
CAC2601		S-adenosylmethionine decarboxylase	1.9	2.1	5.2	3.2	3.1	1.5	E
CAC2702		Possible signal transduction protein	4.0	3.7	3.6	5.0	4.1	0.6	T
CAC2709	etfA	Electron transfer flavoprotein alpha-subunit	2.3	2.0	5.4	2.4	3.0	1.6	C
CAC2711	bcd	Butyryl-CoA dehydrogenase	2.0	1.8	6.1	2.4	3.1	2.0	I
CAC2712	crt	Enoyl-CoA hydratase	2.1	1.8	7.2	2.9	3.5	2.5	I
CAC2810		Glucoamylase family protein	2.7	2.2	10.1	4.9	5.0	3.6	G
CAC2873	thlA	Acetyl-CoA acetyltransferase	2.3	1.7	8.1	3.5	3.9	2.9	I
CAC2938		Hypothetical protein	2.4	1.9	6.5	5.2	4.0	2.2	R
CAC3075	buk	Butyrate kinase	4.0	2.8	8.1	5.7	5.1	2.3	C
CAC3076	ptb	Phosphate butyryltransferase	3.4	2.5	9.5	5.4	5.2	3.1	C
CAC3236		Transcriptional regulator	2.7	2.1	13.2	8.5	6.6	5.3	T,Q
CAC3237	msmX	Sugar ABC transporter, ATP binding protein	2.5	2.2	10.9	8.1	5.9	4.3	G
CAC3379		Hypothetical protein	3.6	3.5	5.6	6.3	4.7	1.4	S
CA_P0036		Uncharacterized, ortholog of YgaT gene of B. subtilis	90.4	19.0	270.0	200.0	144.9	111.8	M
CA_P0037		Uncharacterized, ortholog of YgaS gene of B. subtilis	114.9	54.1	451.9	250.0	217.7	176.3	–
CA_P0038		Uncharacterized conserved protein, YCII family	4.2	3.4	3.2	2.5	3.3	0.7	S
CA_P0072		Hypothetical protein	2.0	2.1	6.0	2.0	3.0	2.0	–
CA_P0073		ABC ATPase containing transporter	2.7	2.4	7.6	2.1	3.7	2.6	V
CA_P0074		Hypothetical protein	2.9	2.2	8.3	2.0	3.9	3.0	–
CA_P0149		Xre family DNA-binding domain and TRP-repeat-containing protein	2.6	2.6	4.2	3.2	3.1	0.8	K

Genes are listed in order of ORFs and considered as significantly induced when the average fold regulation was ≥3.0 and the values in at least three out of four microarrays were ≥2.0

^aProtein names according to Nölling et al. (2001)

^bCluster of orthologous groups (Tatusov et al. 2000)

Two spots with ~4.3-fold and ~4.0-fold increased abundances at pH 5.7 contained mixtures of three different polypeptides each. The first spot comprised three proteins with similar molecular masses (~17.5–18 kDa) and isoelectrical points (pI ~ 4.95–5.27): Hsp18, an 18-kDa heat shock protein (CAC3714), CAC0056, a putative uncharacterized protein, and a transcriptional regulator of the Lrp family (AsnC, CAC0977). Thereof, only cac0056 showed a higher transcript level (~1.5-fold) under these conditions (SD5). The second inhomogeneous spot contained a protein identified as related to the HTH domain of SpoOJ/ParA/ParB/RepB family, involved in chromosome partitioning (CAC0016), a putative S-layer protein (CAC3558), and an ATP phosphoribosyltransferase regulatory subunit (HisZ, CAC0935). The proteins of the latter spot exhibit similar molecular masses (~46–48 kDa) but considerable different isoelectrical points of 5.78 (CAC0016), 6.32 (CAC0935), and 8.26 (CAC3558). Since the pI of CAC3558 was out of the pH range of 4–7 of the used strip, its occurrence was not expected and remains unexplainable.

On the other hand, extracts of solventogenic cells grown at pH 4.5 revealed a total of 29 protein spots to be significantly increased (which are highlighted in Fig. 3 and further information is given in Table 2). Not surprisingly, the gene products of the sol operon (CAP0162–CAP0164), aldehyde alcohol dehydrogenase 1 (AdhE1), and the two subunits of the acetoacetyl coenzyme A:acetate/butyrate:coenzyme A transferase (“CoA-transferase,” CtfA, CtfB) were not detectable at pH 5.7, representing the acidogenic growth. This finding was not unexpected since the respective enzymes are involved in butanol formation, a metabolic pathway which is completely “turned off” (uninduced or repressed) in acidogenic cells. In addition, our array data (see transcriptomic section below) indicated highly elevated transcript levels at pH 4.5 of ~125-fold of the corresponding genes (Table 4 and supplementary data file SD1, Table S2). The protein spots were found in a typical “protein lane” at the right border of the 2-D gels caused by pI values of above 7.0 (AdhE1, 8.44; CtfA, 8.99; CtfB, 7.79; supplementary data file SD3). Thus, during separation in the first dimension, proteins accumulated at the right edge of the strip because it covered a pI range between 4 and 7 only. AdhE1 was detected additionally in numerous smaller “smearing” spots between pI 4.5 and pI 7.0 (SD1, Fig. S2; spot numbers 33, 34, 38–44, 46–47, 50–53 in combination with SD3).

Table 2.

Proteins with increased (≥2.0) abundance in the solventogenesis at pH 4.5

^aProteins of spots with more than one polypeptide are listed in their identification order

^bNames based on Nölling et al. (2001)

^cCorresponding spot numbers in Fig. 2

^cCorresponding spot numbers in Fig. 3

^eThe sign for nonterminating (∞) indicates that the protein was not detectable at pH 5.7

Table 4.

Genes with a significant induction at the transcript level in the solventogenesis

ORF#	Gene	Protein functiona	1. array	2. array	3. array	4. array	Average fold reg.	SD	COGb
CAC0186		Xre family DNA-binding domain and TPR-repeat-containing protein	0.19	0.15	0.24	0.19	0.19	0.04	–
CAC0254	nifHD	Nitrogen regulatory protein PII (nitrogen fixation nifHD)	0.21	0.17	0.53	0.43	0.33	0.17	E
CAC0255	nifHD	Nitrogen regulatory protein PII (nitrogen fixation nifHD)	0.22	0.20	0.41	0.46	0.32	0.13	E
CAC0256	nifD	Nitrogenase molybdenum–iron protein, alpha chain (nitrogenase component I)	0.21	0.16	0.42	0.47	0.32	0.15	C
CAC0392		Peptidoglycan-binding domain	0.30	0.28	0.25	0.36	0.30	0.04	M
CAC0538		ChW repeat-containing mannanase ManB	0.35	0.34	0.24	0.22	0.29	0.07	G
CAC0561		Cellulase CelE-like protein	0.04	0.05	0.11	0.07	0.07	0.03	–
CAC0574		Pectate lyase H (FS)	0.08	0.08	0.19	0.14	0.12	0.05	–
CAC0717		Predicted membrane protein	0.10	0.12	0.15	0.10	0.12	0.02	–
CAC0746		Secreted protease metal-dependent protease	0.14	0.15	0.27	0.25	0.20	0.07	S
CAC0826		Endoglucanase family 5	0.16	0.16	0.29	0.19	0.20	0.06	G
CAC0910		Cellulosomal scaffolding protein	0.007	0.007	0.012	0.007	0.008	0.003	G
CAC0911		Processive endoglucanase	0.007	0.007	0.012	0.010	0.009	0.002	–
CAC0912		Nonprocessive endoglucanase	0.007	0.006	0.013	0.007	0.008	0.003	G
CAC0913		Nonprocessive endoglucanase	0.010	0.008	0.012	0.008	0.009	0.002	–
CAC0914		Cellulosome integrating cohesin-containing protein, secreted	0.009	0.008	0.009	–	0.008	–	–
CAC0915		Endoglucanase A	0.015	0.016	0.010	0.008	0.012	0.004	–
CAC0918		Nonprocessive endoglucanase	0.009	0.007	0.008	0.006	0.008	0.001	–
CAC0919		Sialidase	0.009	0.013	0.013	0.013	0.012	0.002	–
CAC1214		Xre family DNA-binding domain and TPR-repeat-containing protein	0.30	0.25	0.38	0.36	0.32	0.06	–
CAC1314		Hypothetical protein	0.03	0.03	0.04	0.04	0.03	0.002	–
CAC1315		Peptidoglycan-binding domain-containing protein	0.03	0.03	0.04	0.03	0.03	0.004	M
CAC1322	glpA	Glycerol-3-phosphate dehydrogenase	0.06	0.09	0.15	0.08	0.09	0.04	R
CAC1323		NAD(FAD)-dependent dehydrogenase	0.13	0.16	0.29	0.19	0.19	0.07	O
CAC1324		Hypothetical protein	0.13	0.15	0.14	0.19	0.15	0.03	S
CAC1554		Heavy metal-binding domain-containing protein	0.32	0.34	0.30	0.24	0.30	0.05	S
CAC1611		Cation efflux pump (multidrug resistance protein)	0.34	0.33	0.27	0.26	0.30	0.04	V
CAC1673	gltA	Large subunit of NADH-dependent glutamate synthase	0.22	0.26	0.36	0.43	0.32	0.09	E
CAC1968		Pectate lyase related enzyme	0.12	0.11	0.14	0.20	0.14	0.04	–
CAC1977		Predicted membrane protein	0.16	0.19	0.18		0.17	0.02	–
CAC1980		Predicted ATPase involved in pili biogenesis	0.25	0.26	0.28	0.28	0.27	0.01	U
CAC2052		DNA-dependent RNA polymerase sigma subunit	0.24	0.19	0.47	–	0.30	0.15	K
CAC2053		Hypothetical protein	0.27	0.19	0.43	0.26	0.29	0.10	–
CAC2293		Hypothetical protein	0.11	0.19	0.21	0.28	0.20	0.07	–
CAC2392		ABC transporter, ATPase component	0.18	0.19	0.34	0.22	0.23	0.07	V
CAC2393		ABC transporter, ATPase component	0.21	0.18	0.40	0.18	0.24	0.10	V
CAC2396		Xylanase/chitin deacetylase	0.25	0.29	0.29	0.21	0.26	0.04	G
CAC2404		Glycosyltransferase	0.21	0.17	0.20	0.13	0.18	0.03	R
CAC2405		Glycosyltransferase	0.18	0.14	0.28	0.14	0.19	0.07	M
CAC2406		O-antigen transporter permease	0.12	0.16	0.20	0.15	0.16	0.03	R
CAC2407		CheY-like domain-containing protein	0.18	0.15	0.20	0.14	0.17	0.03	T
CAC2408		Glycosyltransferase	0.14	0.12	0.24	0.18	0.17	0.05	M
CAC2450		Desulfoferrodoxin	0.28	0.35	0.27	0.21	0.28	0.06	C
CAC2497		Hypothetical protein	0.17	0.28	0.19	0.22	0.21	0.05	–
CAC2517	nrpE	Extracellular neutral metalloprotease. NPRE	0.06	0.06	0.06	0.04	0.05	0.01	E
CAC2606		Hypothetical protein	0.18	0.19	0.37	0.36	0.28	0.10	G
CAC2607		Gluconate 5-dehydrogenase	0.20	0.19	0.52	0.28	0.30	0.15	I,Q,R
CAC2650	pyrD	Dihydroorotate dehydrogenase	0.15	0.14	0.53	0.38	0.30	0.19	F
CAC2651	pyrZ	Dihydroorotate dehydrogenase electron transfer subunit	0.15	0.13	0.56	0.32	0.29	0.20	H,C
CAC2652	pyrF	Orotidine 5′-phosphate decarboxylase	0.16	0.12	0.63	0.30	0.30	0.23	F
CAC2653	pyrI	Aspartate carbamoyltransferase regulatory subunit	0.21	0.21	0.44	0.33	0.30	0.11	F
CAC2654	pyrB	Aspartate carbamoyltransferase catalytic subunit	0.15	0.12	0.34	0.34	0.24	0.12	F
CAC2920	tenI	Thiamine monophosphate synthase	0.18	0.16	0.52	0.36	0.31	0.17	H
CAC2921	thiH	Thiamine biosynthesis protein ThiH	0.15	0.13	0.56	0.33	0.29	0.20	H,R
CAC2922	thiG	Thiazole synthase	0.15	0.14	0.39	0.24	0.23	0.11	H
CAC2923		Thiamine biosynthesis protein ThiF	0.15	0.14	0.37	0.24	0.23	0.11	H
CAC2924	thiS	Hypothetical protein	0.15	0.15	0.35	0.21	0.22	0.10	H
CAC2928		Predicted membrane protein	0.22	0.15	0.10	0.06	0.13	0.07	S
CAC3166		Predicted DNA-binding protein	0.32	0.27	0.37	–	0.32	0.05	R
CAC3167		Hypothetical protein	0.26	0.20	0.44	0.24	0.29	0.11	S
CAC3276	nrdF	Ribonucleotide-diphosphate reductase beta-subunit	0.38	0.49	0.17	0.14	0.30	0.17	F
CAC3279		ChW repeat-containing protein	0.26	0.28	0.33	0.20	0.27	0.05	N
CAC3280		ChW repeat-containing protein	0.33	0.30	0.34	0.21	0.29	0.06	N
CAC3387		Pectate lyase	0.16	0.17	0.06	0.07	0.11	0.06	–
CAC3469		Endoglucanase family protein	0.05	0.04	0.10	0.06	0.06	0.03	G
CAC3526		FMN-binding protein	0.30	0.22	0.40	0.37	0.32	0.08	–
CAC3612		Hypothetical protein	0.27	0.23	0.22	0.26	0.25	0.03	–
CAC3684		Polygalacturonase	0.21	0.20	0.42	0.27	0.27	0.10	M
CAC3693		Hypothetical protein	0.30	0.41	0.24	0.31	0.31	0.07	–
CAC3694		TPR-repeat-containing protein	0.32	0.37	0.30	0.31	0.32	0.03	R
CAC3695		Transcriptional regulator, containing DNA-binding domain of xre family	0.27	0.30	0.31	0.28	0.29	0.02	–
CAC3696		Hypothetical protein	0.43	0.31	0.30	0.29	0.33	0.07	S
CA_P0004		Cysteine protease	0.02	0.02	0.04	0.04	0.03	0.01	O
CA_P0009		Response regulator	0.25	0.28	0.51	0.24	0.32	0.13	T
CA_P0010	bgla	Beta-glucosidase	0.30	0.32	0.35	0.33	0.32	0.02	G
CA_P0040		Xre family DNA-binding domain and TPR repeats containing protein	0.21	0.19	–	0.26	0.22	0.03	–
CA_P0044		Hypothetical protein	0.18	0.17	0.29	0.19	0.21	0.05	–
CA_P0045		Glycosyl transferase	0.19	0.18	0.23	0.14	0.18	0.04	G,C
CA_P0053	xynb	Xylanase	0.06	0.07	0.05	0.05	0.06	0.01	G
CA_P0054		Xylanase/chitin deacetylase family protein	0.06	0.06	0.06	0.04	0.05	0.01	G
CA_P0056	pell	Pectate lyase	0.10	0.09	0.16	0.11	0.12	0.03	–
CA_P0065		Secreted metalloprotease	0.07	0.07	0.07	0.06	0.06	0.004	–
CA_P0102		Membrane protein	0.11	0.10	0.12	0.08	0.10	0.02	R
CA_P0112		Hypothetical protein	0.27	0.25	0.18	0.17	0.22	0.05	–
CA_P0116		Xylanase	0.17	0.17	0.28	0.28	0.22	0.06	G
CA_P0117		Beta-xylosidase	0.12	0.12	0.22	0.19	0.17	0.05	–
CA_P0118		Xylan degradation enzyme	0.14	0.16	0.18	0.16	0.16	0.02	M
CA_P0119		Xylan degradation enzyme	0.09	0.09	0.15	0.12	0.11	0.03	M
CA_P0120		Xylan degradation enzyme	0.09	0.10	0.16	0.13	0.12	0.03	G
CA_P0128		Permease, MDR related	0.30	0.25	0.05	0.04	0.16	0.13	G
CA_P0129		Glycogen-binding regulatory subunit of S/T protein phosphatase I	0.19	0.21	0.22	0.25	0.22	0.02	–
CA_P0162	adhe1	Aldehyde dehydrogenase	0.012	0.009	0.008	0.004	0.008	0.003	C
CA_P0163	ctfa	Butyrate-acetoacetate CoA-transferase subunit A	0.009	0.010	0.009	0.004	0.008	0.003	I
CA_P0164	ctfb	Butyrate-acetoacetate CoA-transferase subunit B	0.014	0.010	0.007	0.004	0.008	0.004	I
CA_P0168	amyA	Alpha-amylase	0.11	0.09	0.16	0.09	0.11	0.03	G

Genes are listed in order of ORFs and considered as significantly induced when the average fold regulation was ≤0.33 and the values in at least three out of four microarrays were ≤0.5

^aProtein names according to Nölling et al. (2001)

^bCluster of orthologous groups (Tatusov et al. 2000)

Another protein involved in solvent production, NADH-dependent butanol dehydrogenase B (CAC3298, BdhB), was also significantly increased with an infinite ratio as its spot was not detected at pH 5.7 (Table 2). In contrast to the proteins mentioned above, its transcript level was only slightly (~1.7-fold) elevated (SD1, Table S2).

The role of the other proteins found in significantly higher amounts (Table 2) for cells growing at pH 4.5 remains unknown. Interesting examples are carbon monoxide dehydrogenase (CAC0116) which increased up to ~2.1-fold and flagellin FlaC (or hook-associated flagellin protein Hag; CAC2203) which appeared in multiple spots. One of them, spot number 445, was only observed at pH 4.5, indicating a smaller apparent molecular weight and higher pI than expected (SD1, Fig. S2; SD3). In contrast, the two main spots of FlaC revealed considerable higher molecular masses of ~42 kDa with respect to the calculated mass of 29.5 kDa. This phenomenon might be explained by multiple glycosylation (Lyristis et al. 2000).

Other proteins listed in Table 2 represent typical extracellular proteins like an extracellular neutral metalloprotease (CAC2517) or a processive endoglucanase (CAC0911). Increased production at pH 4.5 was in agreement with upregulated transcript levels of ~20-fold and ~111-fold, respectively (Table 4).

Transcriptome analysis

Acidogenic cells and solventogenic cells of a master fermentation were comprehensively compared by DNA microarray analyses. The time points of sampling were identical to those of the proteome analyses (Fig. 1). Complete results are listed in the supplementary data files SD5 and SD6 whereas in Fig. 4 striking differences are highlighted. Accordingly, transcription of 53 genes (1.4%) in acidogenic cells and 95 genes (2.5%) in solventogenic cells was found to be highly upregulated, each in comparison to the status at the other pH value. The majority (66.3%) of the genes did not show significant alterations and further 29.8% showed no transcripts matching the filter criteria (Hillmann et al. 2009).

Fig. 4.

Overview of the transcript levels during acidogenesis at pH 5.7 and solventogenesis at pH 4.5. Log expression ratios of acidogenesis to solventogenesis are shown. All genes with log values (as logarithms to the basis of 2) higher than 1.6 are significantly induced at pH 5.7, and genes with a negative log of less than −1.6 were significantly induced at pH 4.5. According to this definition, all genes between the dashed lines were expected to be not significantly influenced

Genes with increased transcript amounts in acidogenic cells

The detailed results of the 53 open reading frames (ORFs) that revealed at least ≥3.0-fold increase in their transcript levels at pH 5.7 are given in Table 3. Seven of them are located on the megaplasmid pSOL1. Two of them showed particularly high scores of more than 140-fold increase each, cap0036 and cap0037. This finding was in good accordance with the proteome data and prompted us to verify their RNA levels by Northern blot analysis. The cap0036- and cap0037-specific mRNA transcripts were exclusively detected in acidogenic chemostat cells of C. acetobutylicum (Fig. 5). Individual probes against both genes (Fig. 5a, b) revealed signals of the same size of about 1.4 kb, indicating a common transcription unit of a bicistronic operon. More intense hybridization signals using the cap0036 probe may suggest higher mRNA quantities, but a higher hybridization efficiency due to specific base composition and individual nucleotide sequence might also explain the differences.

Fig. 5.

Northern blot analyses of cap0037 and cap0036. Total RNA samples (15 μg per lane in a and b; 1 μg in c) of C. acetobutylicum cells grown at pH 5.7 and pH 4.5 (as indicated) were hybridized with DIG-labeled probes against cap0037 (a), cap0036 (b), or 16S rRNA transcript (c) as control of RNA integrity

The other five genes of pSOL1 with increased transcript levels (approximately threefold to fourfold) comprised the putative operon cap0073 and cap0074 and the putative orphan genes cap0072, cap0038, and cap0149 (Karp et al. 2005). The functions of their gene products are “hypothetical or uncharacterized” although some similarities to a protein of an ABC transporter (CAP0073) or to a DNA-binding domain (CAP0149) have been postulated (Nölling et al. 2001).

Among the chromosomal open reading frames, cac2365 showed the highest transcript increase of ~11-fold at pH 5.7. This gene putatively encodes an SspA-like protein, annotated as a small acid-soluble DNA-binding spore protein which might protect the spore genome. SspA is known to be upregulated in batch cultures of C. acetobutylicum and Clostridium beijerinckii in cells entering stationary growth phase (Jones et al. 2008; Shi and Blaschek 2008). However, C. acetobutylicum did not form spores in exponentially growing cells of continuous chemostat cultures, and its function under these conditions is not clear. Transcriptional induction of SspA might be explained as a consequence of the simultaneous increase (~2.0-fold; SD5) of sigG (CAC1696) because σ^G regulated the synthesis of SspA in Bacillus subtilis (Jones et al. 2008).

Not surprisingly, genes directly responsible for butyrate formation like ptb (CAC3076) and buk (CAC3075) (Hartmanis 1987; Walter et al. 1993; Wiesenborn et al. 1989a) were also strongly induced (approximately fivefold) in acidogenic cells (Table 3, SD1, Table S2). Similarly increased induction was found for genes of enzymes involved in the conversion of acetyl-CoA to butyryl-CoA, e.g., thiolase A (thlA, CAC2873), crotonase (crt, CAC2712), butyryl-CoA dehydrogenase (bcd, CAC2711), and the α subunit of the electron transfer flavoprotein (etfA, CAC2709). Otherwise, 3-hydroxybutyryl-CoA dehydrogenase (hbd, CAC2708) and the second subunit β of the electron transfer flavoprotein (etfB, CAC2710) did not show significantly elevated transcript levels (SD1, Table S2).

Furthermore, seven genes of four different ABC transporter systems were induced at pH 5.7, e.g., a putative ATP binding protein involved in sugar transport (msmX, CAC3237) and the genes cac0427, cac0428, and cac0429 of a glycerol-3-phosphate ABC transporter system which are organized in a common operon together with glycerophosphoryl diester phosphodiesterase (cac0430; Karp et al. 2005). Additionally, ten chromosomal open reading frames (Table 3) encoding unknown “hypothetical proteins” revealed significant higher transcript levels of approximately threefold to ninefold.

Genes with increased transcript amounts in solventogenic cells

The transcript pattern confirmed the proteome studies that in solventogenic cells more genes were found to be upregulated than in acidogenic cells. The mRNA transcripts of 95 genes matched the significance criterion of ≥3.0-fold induction (pH 4.5 versus pH 5.7; Table 4). Particularly, high values (~125-fold) were documented for the genes of the sol operon (cap0162–cap0164) due to the requirement of AdhE1, and the subunits of CoA-transferase are necessary for the production of solvents after the metabolic shift (Fischer et al. 1993; Nair et al. 1994; Wiesenborn et al. 1989b). In addition, similar high levels of the mRNA transcripts of the chromosomal genes cac0910–cac0915 and cac0918–cac0919 were detected. Although glucose represented the single carbohydrate source in the medium, their deduced gene products are likely involved in cellulose degradation (Nölling et al. 2001). Gene products with related functions in xylan degradation (cap0053–cap0054, cap0118–cap0120), a pectate lyase (cap0056), a cellulose CelE-like protein (cac0561), and other endoglucanases (cac0826, cac3469) also showed clearly increased gene expression (~5–20-fold).

Furthermore, transcription of several putative proteolytic enzymes was found to be upregulated between ~5- and 30-fold, e.g., a cysteine protease (cap0004), a secreted metalloprotease (cap0065), a secreted metal-dependent protease (cac0746), and an extracellular neutral metalloprotease NPRE (cac2517). Also, several ORFs with significantly increased transcription at pH 4.5 encode proteins predicted as hypothetical (at least 12) or membrane proteins (at least five) which are encoded by the plasmid pSOL1 (e.g., CAP0044, CAP0102, CAP0112) or the chromosome (e.g., CAC0717, CAC1324, CAC2053, CAC2497), respectively.

Discussion

Several investigations have been conducted to provide useful information on the transcriptome of C. acetobutylicum ATCC824, and limited proteome data are also available (Alsaker and Papoutsakis 2005; Jones et al. 2008; Sullivan and Bennett 2006; Tomas et al. 2003). However, all studies published so far were based on batch cultures with the focus on regulatory aspects of solvent formation and sporulation linked to the transition phase of cell growth. In contrast, exponentially growing cells of a chemostat culture have not been analyzed yet on the molecular level, which constituted the motivation of this study. To accomplish analyses of steady-state cells of C. acetobutylicum reproducibly adapted to the two distinct physiological phases, advantage was taken of continuous cultivation states of C. acetobutylicum for the comparison of acidogenic and solventogenic metabolism as a function of the external pH.

Protein patterns were analyzed by 2-D gel electrophoresis, covering more than 21% of the cytosolic proteins with a pI range of 4–7. This was in good accordance with other proteome reference maps, e.g., 4.6% protein coverage of Corynebacterium glutamicum (Li et al. 2007), 9.8% of Deinococcus geothermalis (Liedert et al. 2009), 16.9% of Corynebacterium jeikeium K411 (Hansmeier et al. 2006), and 21.4% of Bifidobacterium longum (Yuan et al. 2006). However, with respect to a total number of 3,847 annotated protein coding genes of C. acetobutylicum (Nölling et al. 2001), a relatively small fraction of 251 different proteins (6.5%) was identified since only the intracellular fraction of soluble proteins was analyzed and extracellular and insoluble membrane polypeptides were not considered. Furthermore, proteins of a general low abundance might not be detectable due to the limited sensitivity of colloidal Coomassie-stained 2-D gels.

The most interesting proteins identified here were the gene products of cap0036 and cap0037, which appeared as multiple spots on 2-D gels of acidogenic cells. In agreement with the transcriptome data, their high abundance could simply be explained by considerably increased amounts of mRNA at pH 5.7. It is noteworthy that no other transcript in the DNA microarrays showed a similar high induction of more than 200-fold. Northern blot analyses revealed that cap0036 and cap0037 constitute a bicistronic transcription unit with a length of ~1.4 kb, corresponding to the size of both genes plus an 18-b intergenic region and a short 5′ untranslated region (630 b [cap0037] + 729 b [cap0036] + 18 b + UTR = 1,377 b + UTR).

In previous batch cultures, mRNA-transcripts of cap0037/cap0036 were identified in negligible amounts which may be associated with late stationary growth (Alsaker and Papoutsakis 2005; Jones et al. 2008). In 2-D gels presented by Schaffer et al. (2002), the spots of CAP037 and CAP0036 were visible in acidogenic cells as well as in a cell sample referred to as “onset of solventogenesis” which was taken 6 h after the drop of the pH in the chemostat culture of C. acetobutylicum DSM792. Obviously, the time period after the drop of the pH was too short to achieve steady-state solventogenic growth, and CAP0037/CAP0036 still appeared in the protein patterns, preventing a clearly distinguished assignment to acidogenesis.

Unfortunately, the physiological function of CAP0037/CAP0036 could not be deduced. Database searches proposed a transmembrane domain (TMHMM2 program; Krogh et al. 2001) at the C terminus of CAP0037, and alignments with CAP0036 predicted a conserved domain of unknown function belonging to the DUF583 superfamily (Nölling et al. 2001). Orthologous genes seemed to be restricted to Gram-positive bacteria (Karp et al. 2005), and only one clostridial strain, Clostridium difficile, a nonsolvent producer, revealed a homologous gene locus. Orthologs might exist in B. subtilis (ygaS, formerly yhbD), Bacillus thuringiensis, Bacillus cereus, and Bacillus licheniformis. Usually, genes orthologous to cap0037 are accompanied by genes resembling cap0036 (in B. subtilis ygaT, formerly yhbE) found in the same gene order at adjacent positions (exception C. difficile: interchanged gene positions). In contrast to C. acetobutylicum, other bacteria showed one (C. difficile, B. cereus) or up to six genes present in the respective operon (Bacillus anthracis, B. subtilis, Geobacillus thermodenitrificans, B. thuringiensis, Bacillus weihenstephanensis). For example, in B. subtilis, orthologs are located in a three-gene operon (yhbD–yhbE–yhbF; Flórez et al. 2009). The genes yhbD, yhbE, and yhbF were only found among the bacilli and clostridia, which indicates a role in sporulation (Lai et al. 2003). The limited distribution of CAP0037 and CAP0036 suggests a distinct function in C. acetobutylicum. Direct involvement in endospore formation seems questionable because the cultivation conditions applied here explicitly uncoupled solventogenesis and sporulation. This might also be the reason why these proteins have not been noticed in earlier studies employing transient batch cultivation conditions. However, the role of CAP0037/CAP0036 during acidogenic growth and their clear repression during solventogenesis remains to be elucidated.

Regarding significantly induced proteins of steady-state solventogenic cells, the gene products of the sol operon, aldehyde alcohol dehydrogenase (AdhE1) and the subunits of the butyrate-acetoacetate CoA-transferase (CtfA, CtfB) were identified. This correlated well with previous results because the transcription of the sol operon was known to be highly upregulated during batch cultivation at the onset of solvent formation in the stationary growth phase (Alsaker and Papoutsakis 2005; Harris et al. 2002; Jones et al. 2008), and similar expression profiles were also shown in chemostat experiments (Fischer et al. 1993; Fontaine et al. 2002; Sauer and Dürre 1995). On the other hand, further genes coding for enzymes directly involved in solvent production like the NADH-dependent butanol dehydrogenase A (bdhA) and the acetoacetate decarboxylase (adc) did not reveal elevated transcript levels in this study. These genes might show a temporarily limited transcriptional increase coupled to the metabolic switch, corresponding to phase III of the master fermentation (Fig. 1). Accordingly, their expression patterns in steady-state cells before and after the metabolic shift were almost in the same range. Another explanation would be a higher mRNA turnover pushing their amounts below the significance criteria. Several other genes of different functions reported earlier, e.g., genes involved in stress response, branched chain amino acid synthesis, cell motility, and lipid metabolism revealed only marginal differences between acidogenic and solventogenic growth in continuous cultures. It seems likely that their expression maxima during the cell cycle of C. acetobutylicum can be found within a specific time window of the transition phase, i.e., at the onset of solventogenesis (Alsaker and Papoutsakis 2005; Jones et al. 2008; Sauer and Dürre 1995).

The proteins Adc, Bcd, GroEL, GroES, and Hsp18 were found to be highly expressed during the onset of solventogenesis in previous proteome analyses (Schaffer et al. 2002; Sullivan and Bennett 2006), but we did not detect significant differences between the two phases of the chemostat cells growing at pH 5.7 and pH 4.5, respectively, for similar reasons as mentioned above.

Another group of genes induced during the onset of solventogenesis (Alsaker and Papoutsakis 2005; Jones et al. 2008) maintained high expression levels during solventogenic growth of chemostat cultures. Examples are enzymes of xylan and starch metabolism as well as some glycosyltransferases. In theory, glycosyltransferases can be necessary for regulatory purposes, but the increased expression levels of enzymes for xylan and starch metabolism cannot be explained at this point because the synthetic medium used in the chemostat cultures contained a surplus of glucose as single carbon and energy source. Furthermore, referring to the increased expression of putative gene products involved in cellulose degradation (cac0910–cac0915 and cac0918–cac0919), it must be mentioned that C. acetobutylicum cannot utilize cellulose (Lee et al. 1985a) although the genome comprises several genes encoding parts of the cellulosome and its assembly (López-Contreras et al. 2003, 2004; Sabathé et al. 2002). On the other hand, xylanolytic activity of C. acetobutylicum is well known (Lee et al. 1985b), and xylan and xylooligosaccharide hydrolyzing activities were demonstrated for the xylanases CAP0053 (formerly Xyn10A) and CAP0116 (formerly Xyn10B) (Mursheda et al. 2004, 2005).

In general, elaborate proteome analyses require much more time and effort than transcriptome analyses; thus, more DNA microarray data are available for different perturbations affecting the life cycle and solvent production of C. acetobutylicum. Since proteins are more closely linked to the metabolism in the broadest sense than the respective genes, proteomics can be regarded as a more meaningful approach. Nevertheless, both proteome and transcriptome analyses of steady-state cells representing acidogenic and solventogenic growth were used in this study. The general understanding that increased mRNA amounts led to increased protein abundances was confirmed for the majority of the proteins, with CAP0036/CAP0037, the alcohol aldehyde dehydrogenase AdhE1, the CoA-transferase CtfA/B, a neutral metalloprotease (CAC2517), and a processive endoglucanase (CAC0911) as the most significant candidates. However, the global approach including a large number of proteins also revealed several exceptions, e.g., the flagellin FlaC, the seryl-tRNA synthetase SerS1, a Zn-dependent peptidase (CAC3006), and a response regulator (CAC3220) exhibited higher protein abundances at pH 4.5, but the respective transcript levels did not show substantial alteration. Possibly due to increased translation efficiency and/or higher protein stability, similar observations have been reported earlier, e.g., for the C. acetobutylicum glyceraldehyde 3-phosphate dehydrogenase Gap (Schaffer et al. 2002). Contrariwise, some genes revealed significant higher mRNA levels but no or only marginal increases in protein abundance (~1.1-fold to ~1.3-fold). Examples of acidogenic proteins were the acetyl-CoA acetyltransferase (thlA), the enoyl-CoA hydratase (crt), the butyryl-CoA dehydrogenase (bcd), the electron transfer flavoprotein alpha-subunit (etfA), the enoyl-CoA hydratase (buk), and the phosphate butyryltransferase (ptb).

Finally, the protein profiles of the central glycolytic enzymes glucose-6-phosphate isomerase (Pgi), triosephosphate isomerase (Tpi), fructose-bisphosphate aldolase (Fba), glyceraldehyde 3-phosphate dehydrogenase (GapC), phosphoglycerate kinase (Pgk), phosphoglyceromutase (Pgm), and pyruvate kinase (PykA) showed no significant differences in acidogenesis and solventogenesis and correlated well with their mRNA levels.

In conclusion, novel reference maps of C. acetobutylicum acidogenic and solventogenic proteins with a maximum degree of reproducibility were generated from steady-state cells of chemostat cultures. The proteome maps and accompanying transcriptome analyses constitute a reliable basis for various future investigations to specifically alter endogenous (e.g., certain mutant strains) or exogenous (e.g., defined nutrients) parameters. Another clear advantage of the approach presented here was the strict uncoupling of solventogenesis and sporulation which allows the identification of candidate proteins distinctly related to the metabolic shift. Whether the striking acidogenic proteins CAP0037 and CAP0036 play a major role in the switch between acidogenic and solventogenic metabolism remains to be investigated. Moreover, the generated data sets provide a useful fundamental for systems biology projects such as the European COSMIC project (C. acetobutylicum systems microbiology, http://www.sysmo.net) to assess the biotechnological impact of C. acetobutylicum as a superior solvent production strain.