Open Access

The alternative sigma factor SigB of Corynebacterium glutamicum modulates global gene expression during transition from exponential growth to stationary phase

  • Christof Larisch1,
  • Diana Nakunst1,
  • Andrea T Hüser1,
  • Andreas Tauch1 and
  • Jörn Kalinowski1Email author
BMC Genomics20078:4

DOI: 10.1186/1471-2164-8-4

Received: 08 September 2006

Accepted: 04 January 2007

Published: 04 January 2007

Abstract

Background

Corynebacterium glutamicum is a gram-positive soil bacterium widely used for the industrial production of amino acids. There is great interest in the examination of the molecular mechanism of transcription control. One of these control mechanisms are sigma factors. C. glutamicum ATCC 13032 has seven putative sigma factor-encoding genes, including sigA and sigB. The sigA gene encodes the essential primary sigma factor of C. glutamicum and is responsible for promoter recognition of house-keeping genes. The sigB gene codes for the non-essential sigma factor SigB that has a proposed role in stress reponse.

Results

The sigB gene expression was highest at transition between exponential growth and stationary phase, when the amount of sigA mRNA was already decreasing. Genome-wide transcription profiles of the wild-type and the sigB mutant were recorded by comparative DNA microarray hybridizations. The data indicated that the mRNA levels of 111 genes are significantly changed in the sigB-proficient strain during the transition phase, whereas the expression profile of the sigB-deficient strain showed only minor changes (26 genes). The genes that are higher expressed during transition phase only in the sigB-proficient strain mainly belong to the functional categories amino acid metabolism, carbon metabolism, stress defense, membrane processes, and phosphorus metabolism. The transcription start points of six of these genes were determined and the deduced promoter sequences turned out to be indistinguishable from that of the consensus promoter recognized by SigA. Real-time reverse transcription PCR assays revealed that the expression profiles of these genes during growth were similar to that of the sigB gene itself. In the sigB mutant, however, the transcription profiles resembled that of the sigA gene encoding the house-keeping sigma factor.

Conclusion

During transition phase, the sigB gene showed an enhanced expression, while simultaneously the sigA mRNA decreased in abundance. This might cause a replacement of SigA by SigB at the RNA polymerase core enzyme and in turn results in increased expression of genes relevant for the transition and the stationary phase, either to cope with nutrient limitation or with the accompanying oxidative stress. The increased expression of genes encoding anti-oxidative or protection functions also prepares the cell for upcoming limitations and environmental stresses.

Background

The RNA polymerase of prokaryotic organisms is composed of distinct subunits: β, β', ω, an α dimer, and a σ factor [1]. The sigma factor of the RNA polymerase confers specificity to the process of transcription initiation by recognition of specific promoter sequences of genes and operons [2]. Under normal growth conditions, bacteria use generally a RNA polymerase holoenzyme containing the principal sigma factor SigA. This sigma factor is essential for the transcription of house-keeping genes [3]. It is generally observed that under nutrient limitation or under a variety of physical and chemical stresses, additional sigma factors compete for the limited amount of RNA polymerase core enzyme. These sigma factors are non-essential for exponential growth and fall into different families. The first family comprises sigma factors of the non-essential sigma factors subgroups 2.1 from gram-negative bacteria, such as σS from Escherichia coli, and 2.3 comprising the σB factors from gram-positive Actinobacteria [4]. These sigma factors are similar to the primary sigma factor in the amino acid sequence of the DNA-binding region, which suggests that both groups of sigma factors recognize similar promoter sequences [5, 6]. The other family comprises alternative sigma factors of the subgroup 3.3, such as σB of Bacillus subtilis and related gram-positive Firmicutes [7] which recognize promoters with a different consensus sequence [4].

In gram-negative bacteria like E. coli the non-essential sigma factor σS (RpoS) is strongly induced during entry into the stationary phase as well as under stress conditions and is essential for the expression of multiple stress resistance genes [8]. In Mycobacterium tuberculosis, the non-essential sigma factor σB behaves like σS of E. coli [9] since its transcription is induced during transition from exponential to stationary phase and under certain stress conditions. Therefore, it has been suggested that RpoS and mycobacterial SigB play similar roles in the general stress response of gram-negative and gram-positive bacteria [10]. In B. subtilis, the unrelated alternative sigma factor σB regulates the transcription of a large number of general stress operons, thereby contributing to the transcription of more than 200 genes involved in heat, acid, ethanol, salt, and oxidative stress resistance [11, 12].

Corynebacterium glutamicum is a gram-positive non-pathogenic soil bacterium widely used for the production of amino acids. There is great interest in the examination of amino acid biosynthesis pathways and the molecular mechanism of transcription control [13, 14]. One of these control mechanisms at the transcriptional level are sigma factors. Annotation of the genome sequence of C. glutamicum ATCC 13032 revealed the presence of seven putative sigma factor genes, including sigA and sigB [15, 16]. The sigA gene encodes the essential primary sigma factor of C. glutamicum and is responsible for promoter recognition of house-keeping genes [17, 18]. The nucleotide sequence of the -10 region of the SigA consensus promoter sequence is tgngnTA(c/t)aaTgg [19]. The sigB gene encoding the non-essential sigma factor SigB is transcribed during the exponential growth phase and transcript abundance ceases in stationary phase [20]. Halgasova et al. [21] showed that SigB is involved in the response to several environmental stresses, such as acids, ethanol, cold, and heat shock and that disruption of the sigB gene leads to a substantially diminished growth of the mutant in shake-flask cultures. In this study, we analyzed by DNA microarray hybridizations the role of SigB during the transition of C. glutamicum growth phases to get a detailed and genome-wide view on the modulation of gene expression.

Results

The growth behavior of both a sigB-deficient and sigB-proficient C. glutamicum strains was comparable under controlled cultivation conditions in glucose-limited batch fermentations

To investigate the physiological role of the sigma factor SigB in C. glutamicum, a sigB deletion mutant was constructed by gene replacement in C. glutamicum RES167, a restriction-deficient derivative of the wild-type strain ATCC 13032, and designated C. glutamicum CL1. The deletion introduced into the sigB gene was 771 bp in size and removed the coding sequence for 257 of the 331 amino acids, including the highly conserved protein regions 1, 2 and 3 of sigma factor proteins [22].

A glucose-limited batch fermentation was chosen for cultivation of both the sigB-proficient strain C. glutamicum RES167 and the sigB-deficient strain C. glutamicum CL1. The cultures were grown at 30°C in a fermentor with a constant pO2 level of 30% and a pH of 7. Beside the impeller speed, carbon dioxide production was monitored online, and the remaining glucose was determined by off-line measurements. The time point of glucose exhaustion and the transition from exponential to stationary phase are precisely defined by an immediate drop in carbon dioxide production at glucose exhaustion (data not shown). Under these conditions, the growth profiles of both cultures (Fig. 1) were similar and also the maximal growth rates differed only slightly (RES167: 0.22 ± 0.03 h-1; CL1: 0.27 ± 0.02 h-1).
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Figure 1

Growth and sugar consumption during batch-fermentation of C. glutamicum RES167 (black squares) and the sigB mutant C. glutamicum CL1 (open squares) in minimal medium MM1 at 30°C and pH 7. Growth was monitored by measuring the optical density (o.D.) at a wavelength of 600 nm. Black triangles symbolize the remaining glucose in cultures of C. glutamicum RES167, open triangles show the glucose concentration in cultures of the sigB mutant C. glutamicum CL1. The numbers correspond to different sampling points of C. glutamicum RES167 and C. glutamicum CL1 cells for further analyses.

The C. glutamicum sigB gene encoding an alternative sigma factor was preferentially transcribed during transition from exponential growth to stationary phase

To determine whether the sigma factor gene expression is influenced by the growth phase of C. glutamicum cultures, transcription profiles of the sigA gene encoding the house-keeping sigma factor and of the sigB gene were recorded. Both strains were cultivated in the controlled environment of a fermentor minimizing the influence of environmental stresses and differences in growth rates between both strains. The transition phase was induced in a reproducible manner by limiting the carbon source glucose. Thus, C. glutamicum RES167 and CL1 cells were harvested during exponential growth phase (Fig. 1; sample number 1 to 6), during transition phase (sample number 7 and 8) and during the stationary growth phase (sample number 9 and 10). The sample numbers correspond to the different growth phases of C. glutamicum cells for all further analyses. The amounts of sigA and sigB transcripts were then determined by real-time RT-PCR. Figure 2A shows the relative amounts of sigA and sigB transcripts in C. glutamicum RES167 at different points of the growth profile in comparison to those determined at mid-exponential phase (time point 4 in Fig. 1).
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Figure 2

Relative levels of sigA and sigB mRNA in C. glutamicum RES167 at different phases of growth. (A) The bars show mRNA levels of sigA (solid bars) and sigB (speckled bars) calculated in relation to those determined at early exponential growth phase in the wild-type. The sample numbers correspond to the sampling points marked in Figure 1. (B) The bars show mRNA levels of the sigA gene in the sigB-deficient C. glutamicum strain CL1.

The analysis indicated that sigA is almost constantly transcribed during the exponential growth phase. Such an expression pattern has been reported also for the main sigma factor σ70 of E. coli [2]. At transition phase (sample number 8), a significant decline in abundance of sigA mRNA was observed in C. glutamicum RES167 (Fig. 2A). The sigB mRNA abundance was highest at the transition phase (sample numbers 7 and 8) and, unlike to that of sigA, remained at an increased level in early stationary phase (sample number 9). At later stages of the stationary phase the sigB mRNA level decreased (Fig. 2A). The mRNA levels of sigA were also determined for the sigB-deficient C. glutamicum mutant strain CL1 (Fig. 2B). Surprisingly, the expression of sigA remained at identical levels during exponential growth and transition phase (sample number 8), whereas a decreased expression was observed again in early and late stationary phase (sample numbers 9 and 10).

Global gene expression of a sigB-proficient and a sigB-deficient C. glutamicum strain differed significantly during transition phase

The sigB-proficient strain RES167 and its derived sigB-deficient deletion mutant CL1 were used to identify genes that are transcribed under the control of SigB by microarray hybridization.

In total, three different microarray experiments were carried out. In the first experiment, the global gene expression of the sigB-proficient strain RES167 was compared to that of the sigB-deficient strain CL1 whereby both strains were harvested in the exponential growth phase (sample number 4). This experiment should clarify whether SigB plays a role in global gene expression in the exponential growth phase. In the second experiment, the global gene expression of the sigB-proficient strain RES167 was compared between the transition growth phase (sample number 8) and exponential growth phase (sample number 4). This experiment was designed to monitor the changes in the global gene expression of the sigB-proficient strain between the exponential and the transition growth phase. In the third experiment, the global gene expression of the sigB-deficient strain CL1 was compared between the same two growth phases, namely the exponential growth phase (sample number 4) and the transition growth phase (sample number 8). The third experiment had the same design as the second one with the only difference that the sigB-deficient strain was analyzed. Genes that were found differentially expressed in this experiment are apparently regulated independently of SigB.

For microarray analyses, C. glutamicum RES167 and CL1 cells were harvested during exponential phase (Fig. 1; sample number 4) or during transition phase (sample number 8), respectively. Total RNA samples were prepared from two independently grown cultures of each strain at the two time points and each RNA preparation was used in two hybridization assays, applying label-swapping. Therefore, differential gene transcription was determined by four DNA microarray hybridizations and a total of 16 gene replicates. Labeling of probes, array hybridization and data evaluation were carried out as described previously [23]. Normalization by the LOWESS function and t-test statistics were accomplished with the EMMA microarray data analysis software [24]. In all experiments, an m-value cut-off of ± 1.0, corresponding to relative expression changes equal or greater than 2, was applied.

In the first experiment (RES167/exp vs. CL1/exp), no gene was detected that delivered a significant change in gene expression (data not shown). This indicated that the absence of SigB did not result in differential gene expression during exponential growth phase and that the transcription of sigB in the exponential phase of the C. glutamicum RES167 strain has no effect during the exponential growth phase, too. This experiment allowed us to compare the results of the two following experiments directly.

In the second experiment (RES167/trans vs. RES167/exp), a total number of 111 genes revealed differential expression, including 66 genes with significantly increased expression (e.g. bioY,bioB, bioA and aroF) and 45 genes with decreased expression in the transition phase (e.g. seuC, seuB, ssuD2, ssuC, ssuD1 and ssuB) (Fig. 3A). In the third experiment (CL1/trans vs. CL1/exp), 26 genes had a different expression level in transition phase, including 10 genes with increased expression (bioB, bioY and phoD) and 16 genes with decreased expression (e.g. seuC, seuB, ssuD2, ssuC, ssuD1 and ssuB) (Fig. 3B). This experiment demonstrates, that in the strain C. glutamicum CL1 fewer genes were differentially expressed during the transition growth phase.
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Figure 3

Identification of SigB-dependent genes by DNA microarray hybridization. Ratio/intensity (m/a) plots of DNA microarray hybridizations of sigB-proficient C. glutamicum RES167 (A) and sigB-deficient C. glutamicum CL1 (B) comparing genome-wide transcription at transition phase with that at early exponential phase. Diamonds represent genes with enhanced mRNA levels during transition phase; triangles represent genes with decreased mRNA levels. Each data point was calculated as the average of two biological and two technical replicates including dye-swapping. Selected genes, which were discussed in the text, are indicated (C) The diagram shows the numbers of genes with enhanced and reduced expression during transition phase in the sigB-proficient strain C. glutamicum RES167 (left), the sigB-deficient strain C. glutamicum CL1 (right) and in both strains (middle).

These data sets enabled us to classify all genes according to their expression behavior in the latter two experiments (Fig. 3C): the first class comprises genes with altered mRNA levels at transition phase in C. glutamicum RES167, compared to those showing altered mRNA levels during transition phase in C. glutamicum CL1. In total, 58 genes were identified that revealed an enhanced transcription during transition phase and 37 genes had decreased mRNA levels at transition phase only in the presence of a functional sigB gene (Table 1). The genes of the first class can be considered as being transcribed with the help of SigB, whereas those of the second class require other explanations. They might either be influenced by transcriptional regulators that are expressed with the help of SigB or might be transcribed by another sigma factor and are therefore sensitive to the lowered amount of free RNA polymerase holoenzyme.
Table 1

Genes with significantly altered expression at transition phase only in the sigB-proficient C. glutamicum strain (RES167).

CDS

Gene name

Predicted function

m-value

AMINO ACID METABOLISM AND PROTEOLYSIS

cg0998

 

trypsin-like serine protease

1.57

cg1129

aroF

phospho-2-dehydro-3-deoxyheptanoate aldolase

1.87

cg1783

soxA'

glycine/D-amino acid oxidase – fragment

1.16

cg1930

 

secreted trypsine-like serine protease

1.29

cg2418

ilvE

branched-chain amino acid aminotransferase

1.48

cg2884

 

dipeptide/tripeptide permease

1.21

cg1453

leuB

3-isopropylmalate dehydrogenase

-1.04

cg2588

proB

glutamate 5-kinase protein

-1.43

CARBON METABOLISM AND TRANSPORT

cg1479

glgP1

glycogen phosphorylase

1.17

cg2796

 

MmgE/PrpD family protein

1.19

cg0699

guaB2

inositol-monophosphate dehydrogenase, CBS domain

-1.07

cg0756

cstA

putative carbon starvation protein A

-1.61

cg0812

dtsR1

acetyl/propionyl-CoA carboxylase beta chain

-1.24

cg1790

pgk

phosphoglycerate kinase

-1.06

cg1791

gap

glyceraldehyde-3-phosphate dehydrogenase

-2.01

cg2704

 

sugar ABC-transporter, permease component

-1.38

cg2705

amyE

sugar ABC-transporter, binding protein

-1.42

cg3096

 

aldehyde dehydrogenase

-1.17

cg3219

ldh

L-lactate dehydrogenase

-1.10

cg3380

 

short-chain dehydrogenase

-1.06

STRESS DEFENSE MECHANISMS

cg1028

 

restriction-modification system, methylase

1.04

cg0291

 

intradiol ring-cleavage dioxygenase

1.90

cg1073

 

glyoxylase

1.06

cg2078

 

methionine-R-sulfoxide reductase

1.09

cg2999

 

FAD-dependent oxidoreductase

1.12

cg3141

hmp

flavohemoprotein involved in NO detoxification

1.61

cg1595

uspA2

universal stress protein UspA

-1.11

cg3100

dnaK

heat shock protein Hsp70

-1.58

MEMBRANE PROCESSES

cg0465

 

conserved hypothetical membrane protein

1.21

cg0467

 

cobalamin/Fe3+-siderophores transport system

1.22

cg1082

 

putative membrane protein

1.39

cg1130

uppS1

undecaprenyl pyrophosphate synthetase

1.50

cg1344

narG

nitrate reductase 2, alpha subunit

1.01

cg1345

narK

nitrate/nitrite transporter

1.36

cg1622

 

ABC-type multidrug/protein/lipid transport system

1.06

cg1623

 

divalent heavy-metal cations transporter

1.18

cg2215

 

membrane protein

1.25

cg2377

mraW

S-adenosylmethionine-dependent methyltransferase

1.03

cg2425

 

permease

1.01

cg2440

 

permease

1.23

cg2676

 

ABC-type peptide/nickel transport system

1.18

cg2810

 

Na+/H+-dicarboxylate symporter family

1.43

cg3337

 

putative membrane protein

1.18

cg3338

 

putative membrane protein

1.04

cg1108

porC

putative porin precursor

-1.25

cg1109

porB

anion-specific porin precursor

-1.84

cg1349

 

membrane protein, CBS domain

-1.79

cg1639

 

membrane protein, CBS domain

-1.23

cg1640

 

membrane protein, CBS domain

-1.52

cg2467

 

ABC-transporter ATP-binding protein

-1.33

cg2468

 

ABC-transporter permease component

-1.26

cg2511

 

putative membrane protein

-1.80

cg3175

 

membrane protein

-1.36

cg3195

 

flavin-containing monooxygenase involved in K+ transport

-1.16

PHOSPHORUS METABOLISM AND REGULATION

cg0866

 

phosphoribosyl transferase

1.02

cg1718

 

phospholipid-binding protein

1.02

cg2842

phoU

phosphate uptake regulator

1.31

cg2888

phoR

phosphate starvation two component response regulator

1.11

cg3194

 

membrane-associated phosphoesterase

1.06

cg2513

phoH2

phosphate starvation-inducible protein

-1.22

REGULATORY PROCESSES

cg1083

cgtS10

probable two component sensor kinase

1.23

cg1084

cgtR10

two component response regulator

1.47

cg2614

 

bacterial regulatory proteins, TetR family

1.18

cg3230

 

transcriptional regulator, λ repressor-like

1.13

TRANSCRIPTION AND TRANSLATION

cg0572

rplJ

50S ribosomal protein L10

-1.43

cg0573

rplL

50S ribosomal subunit protein L7/L12

-1.37

cg2092

sigA

RNA polymerase sigma 70 factor

-1.03

VITAMINS/COFACTORS BIOSYNTHESIS AND TRANSPORT

cg0999

 

molybdenum cofactor biosynthesis protein

1.02

cg1132

coaA

pantothenate kinase

1.11

cg0899

 

glutamine amidotransferase/pyridoxine biosynthesis

-1.29

FUNCTION UNKNOWN

cg0096

 

conserved hypothetical protein

3.08

cg0097

 

conserved hypothetical protein

2.57

cg0753

 

secreted protein

1.04

cg0806

 

conserved hypothetical protein

1.20

cg0935

 

conserved hypothetical protein

1.28

cg1091

 

hypothetical protein

1.85

cg1131

 

conserved hypothetical protein

1.59

cg1286

 

conserved hypothetical protein

1.55

cg1304

 

secreted protein

1.58

cg1417

 

GCN5-related N-acetyltransferase

1.41

cg2057

 

secreted protein

1.35

cg2105

 

conserved hypothetical protein

1.14

cg2797

 

conserved hypothetical protein

1.21

cg2850

 

conserved hypothetical protein

1.14

cg3022

 

conserved hypothetical protein

1.15

cg3329

 

conserved hypothetical protein

1.09

cg3330

 

putative secreted protein

1.71

cg0177

 

hypothetical protein

-1.21

cg0757

 

conserved hypothetical protein

-1.20

cg0838

 

DEAD-box helicase

-1.05

cg0892

 

conserved hypothetical protein

-1.03

cg1013

 

hypothetical protein

-1.30

cg1167

 

putative secreted protein

-1.14

cg1911

 

putative secreted protein

-1.07

cg2464

 

conserved hypothetical protein

-1.32

For defining the second class, genes differentially expressed in transition phase independent of SigB were identified (Table 2). A closer inspection of these genes revealed that they essentially belong to two different functional complexes. First, these were the biotin biosynthesis and transport genes cg0095 (bioB), cg2147 (bioY)-cg2149, cg2885 (bioA) cg2886 (bioD) which were all found stronger expressed in transition phase in the sigB-proficient and the sigB-deficient strain. This expression pattern indicates an additional biotin limitation in the fermentation, since biotin had to be added as a supplement due to an auxotrophy of C. glutamicum [25]. Second, the genes and operons involved in utilization of sulfonates and sulfonate esters as sulfur sources cg1147 (ssuI)-cg1156 (ssuD2), cg1376(ssuD1)-cg1379(ssuB) [26], are all downregulated in transition growth phase. This can be interpreted as the reflection of a higher concentration of free sulfate or sulfite in the cell at transition growth phase since these substances are known to inactivate the transcriptional activator of these genes, SsuR [27].
Table 2

Genes with significantly altered expression at transition phase in sigB-proficient C. glutamicum strain (RES167) and its derived sigB-deficient mutant (CL1).

CDS

Gene name

Predicted function

m-value RES167

m-value CL1

BIOTIN BIOSYNTHESIS AND TRANSPORT

cg0095

bioB

biotin synthase

3.69

1.55

cg2147

bioY

membrane protein, BioY family

3.70

1.51

cg2148

 

ABC transporter, ATP-binding protein

3.11

1.51

cg2149

 

permease (cobalt permease subfamily)

1.63

0.75*

cg2885

bioA

adenosylmethionine-8-amino-7-oxononanoate aminotransferase

2.09

0.91*

cg2886

bioD

dethiobiotin synthetase protein

1.32

0.76*

cg1227

 

ABC-type cobalt transport system

1.58

1.48

FUNCTION UNKNOWN

cg0378

 

putative phage-associated protein

1.14

1.61

SULFONATE (ESTER) METABOLISM AND TRANSPORT

cg1147

ssuI

reductase involved in sulfonate degradation

-1.25

-1.70

cg1152

seuB

sulfonate ester monoxygenase

-1.35

-1.25

cg1153

seuC

sulfonate ester monooxygenase

-0.99*

-1.07

cg1156

ssuD2

alkanesulfonate monooxygenase

-2.23

-1.00

cg1376

ssuD1

alkanesulfonate monooxygenase

-2.11

-1.61

cg1377

ssuC

aliphatic sulfonates ABC transporter

-2.17

-1.32

cg1379

ssuB

aliphatic sulfonates ABC transporter

-1.75

-0.74*

CELL DIVISION

cg2378

mraZ

MraZ protein

-1.02

-1.16

* m-values below the set cut-off are indicated in the case of proven or predicted operons

A very small number of genes showed differential expression at transition phase only in the sigB mutant strain (data not shown). Since these genes display rather small ratios and their gene products have not been studied in C. glutamicum, they will not be discussed further.

Classification of genes differentially transcribed only in the sigB-proficient C. glutamicum strain

The genes that display differential expression in the transition growth phase only in the presence of sigB were ordered into nine functional classes according to the annotation of their gene products (Table 1). The first class Amino Acid Metabolism and Transport comprises genes encoding proteolytic enzymes (cg0998, cg1930) and the uptake of peptides (cg2884) which are all found to be upregulated. In addition, genes encoding the first step of aromatic amino acid biosynthesis (aroF) and the final step in aromatic and branched-chain amino acid biosynthesis (ilvE) are upregulated. In contrast to this, the gene encoding the first step in proline biosynthesis (proB) and second second-last step in leucine biosynthesis (leuB) are found to be downregulated. The gene products of leuB and ilvE encode consecutive reactions in leucine biosynthesis having the common intermediates 2-oxo-4-methyl-3-carboxy-pentanoate and 4-methyl-2-oxopentanoate which is a spontaneously occurring decarboxylation product.

It is interesting to note that only few genes involved in the second functional class Carbon Metabolism and Transport were upregulated depending of sigB. Among these genes is cg1479 (glgP1) which encodes a putative glucan phosphorylase responsible for the mobilization of carbon storage reserves such as glycogen. Other genes involved in carbon metabolism, like cg0756 (cstA), which encodes a putative carbon starvation protein, cg1791 (gap) and cg1790 (pgk), which encode glyceraldehyde-3-phosphate dehydrogenase and phosphoglycerate kinase taking part in glycolysis, respectively, are repressed during transition phase. Both genes are located together in an operon of the order gap-pgk-tpi-ppc further encoding triose-phosphate isomerase and PEP carboxylase, respectively [28]. In addition, further genes encoding putative enzymes involved in carbon metabolism or in the uptake of sugars (cg0699, cg2705/amyE-cg2704) were found to be repressed in the sigB-proficient strain.

In the third class Stress Defense Mechanisms the picture is the opposite. Here a considerably high number of putative detoxification genes encoding glyoxlase (cg1073), methionine-R-sulfoxide reductase (cg2078) or the nitric oxide-detoxification flavohemoprotein (hmp) were found to be upregulated. In contrast to this, only the genes encoding a putative universal stress protein (uspA2) and the chaperone Hsp70 (dnaK) were downregulated.

A high number of genes coding for proteins involved in Membrane Processes are differentially regulated in transition phase. Here the picture is not very clear but the genes involved in processes like metal uptake (cg0467, cg1623, cg2676) or cell wall lipid carrier biosynthesis (uppS1) were found to be upregulated whereas those encoding other membrane proteins or the two porins (porB, porC) were downregulated. It is interesting to note that three of the membrane proteins containing the energy-sensing CBS-domain [29] were downregulated, too.

The class Phosporus Metabolism and Regulation largely comprises genes found to be upregulated. These genes apparently encode functions involved in phospholipid metabolism (cg1718, cg3194) and regulation of phosphate uptake or the phosphate starvation response (phoU, phoR). In E. coli the PhoU protein senses the concentration of intracellular inorganic phosphate and is a negative regulator of organophosphate uptake and polyphosphate formation [30]. The C. glutamicum phoR gene encodes the transcriptional regulator of the recently discovered two-component regulatory system PhoRS [31] and is supposed to activate transcription of genes necessary for survival under low phosphorus concentrations. However, none of the genes differentially regulated in dependence on sigB is a member of the regulon reacting on the intracellular inorganic phosphate level [32].

The sixth class Regulatory Processes comprises four genes with induced transcription. These encode another two-component sensor/regulator system (cgtS10, cgtR10), a TetR-type and a λ repressor-like transcriptional regulator. Unfortunately, it is not known which signals trigger these regulators or which genes are regulated by them. They might be among those that are differentially regulated only in the sigB-proficient strain.

The class Transcription and Translation includes three genes, which are all downregulated. The rplJ and rplL genes lie together in an operon and encode the ribosomal protein subunits L10 and L7/L12. The same growth phase-dependent transcription of the rplJL operon showing a decrease at transition phase was already shown for another actinomycete, Streptomyces coelicolor [33]. The third gene in this category is sigA encoding the essential house-keeping sigma factor SigA. In concordance with the transcription profiles established by RT-PCR before, the sigA transcript was found to be less abundant in transition growth phase when a functional sigB gene is present. This is an indication that the apparent downregulation of some genes during transition phase is an indirect consequence of the higher level of sigB expression.

In the class Vitamins/Cofactors Biosynthesis and Transport, three genes involved in different cofactor synthesis pathways are placed. The gene coaA encodes pantothenate kinase, catalyzing the first step of coenzyme A biosynthesis [34] and being upregulated at transition phase. Another gene involved in pyridoxine biosynthesis was upregulated (cg0999), whereas a third gene involved in molybdenum cofactor biosynthesis was found to be downregulated (cg0899). Here no consistent regulatory pattern was apparent.

The class Function Unknown comprises 25 genes the products of which are present also in other bacteria (conserved hypothetical proteins) but have only an ill-defined or entirely unknown function. The larger fraction of these genes or operons was found to be upregulated in the presence of sigB.

Mapping of promoters in front of genes showing an elevated expression in the sigB-proficient C. glutamicum strain at transition phase

RACE-PCR assays were performed to determine the promoter sequences of the six genes/operons cg0096/cg0097, cg1083 (cgtS10)/cg1084 (cgtR10), cg1417, cg2418 (ilvE), cg3141 (hmp), and cg3330. These genes were selected because their mRNA abundances showed high ratios during the transition phase only in the presence of SigB. The RACE-PCR was performed by using total RNA of C. glutamicum RES167 harvested during transition phase, and the transcriptional start sites were determined by comparison to the whole genome sequence [16]. The results of promoter mapping are shown in Figure 4. The deduced -35 and -10 promoter sequences of the investigated genes were indistinguishable from the consensus promoter sequence of C. glutamicum [19].
https://static-content.springer.com/image/art%3A10.1186%2F1471-2164-8-4/MediaObjects/12864_2006_Article_717_Fig4_HTML.jpg
Figure 4

Promoter sequences of C. glutamicum genes showing elevated expression at the onset of stationary phase. The transcription start sites mapped by RACE PCR assays are shown in boldfaced, capital letters. The numbers indicates the position of the transcription start site relative to the translational start codon. The deduced -10 sequences are shown in bold, the -35 elements are underlined. Nucleotides that match the proposed consensus for the -10 element of C. glutamicum are symbolized by capital letters. The consensus sequence of the -10 element of the C. glutamicum sigma factor SigA [tgngnTAtaaTgg] is shown for comparison [19].

Expression profiles of genes showing an elevated expression in the sigB-proficient C. glutamicum strain at transition phase

Furthermore, transcription profiles of sigB, cg0096, cg1083, cg1417, cg2418, cg3141, cg3330, sigA, hom, and gap were determined by real-time RT-PCR during growth of C. glutamicum RES167. The house-keeping genes sigA, hom (encoding homoserine dehydrogenase) and gap (encoding glyceraldehyde-3-phosphate dehydrogenase) served as controls since they are known to be transcribed by SigA [19]. Transcription profiles of cg0096, cg1083, cg1417, cg2418, cg3141, and cg3330 in the sigB-proficient background of C. glutamicum RES167 were very similar to that of sigB during different growth phases (Fig. 5A). In the sigB mutant C. glutamicum CL1, these profiles changed and were apparently different to those of C. glutamicum RES167, especially during transition phase (Fig. 5B). However, the expression profiles of the selected genes of C. glutamicum CL1 became very similar to those of the SigA-transcribed genes sigA, hom and gap of C. glutamicum RES167 (Fig. 5C).
https://static-content.springer.com/image/art%3A10.1186%2F1471-2164-8-4/MediaObjects/12864_2006_Article_717_Fig5_HTML.jpg
Figure 5

Real-time RT-PCR analysis of relative transcription levels of sigB, cg0096, cg1083, cg1417, cg3141, cg3330, cg2418, sigA, hom, and gap during growth. The sample numbers refer to the growth curves shown in Figure 1. Transcription levels were calculated relative to sample number 4 (early exponential phase). The diagrams show gene expression in the sigB-proficient strain C. glutamicum RES167 (A) and in the sigB-deficient strain C. glutamicum CL1 (B). Diagram (C) shows relative expression levels of known SigA-dependent genes of C. glutamicum RES167.

Discussion

SigB is involved in regulation of transition from exponential growth to stationary phase

Our data revealed that SigB is not only necessary for stress response, but also for growth phase-dependent gene regulation. After batch fermentation of the sigB-proficient and sigB-deficient C. glutamicum strain, the generation time of both were rather similar. These results were in contrast to those of Halgasova et al. who recorded a severe growth defect of a sigB-disrupted C. glutamicum mutant [21]. The main difference between both experimental approaches is apparently the method of cultivation. We employed a fermentor for the cultivation of C. glutamicum strains and thus avoided specific stress conditions that might result in growth deficiency of a sigB mutant as observed during cultivation in shake-flasks without aeration and pH control [21]. This notion is supported by the previous observation that expression of the sigB gene increased after supplying a number of environmental stress conditions to C. glutamicum cultures. However, it remains to be investigated whether occasional stress in shaking-flask cultures such as shifting pH or limited dissolved oxygen is a trigger for SigB activity. Furthermore, the transcription analysis of sigA and sigB clarified the different dependency of expression during different growth phases. Real-time RT-PCR analysis showed that transcription of the sigB gene was significantly increased when C. glutamicum entered the transition growth phase. This finding supports the assumption that SigB is the alternative sigma factor of C. glutamicum and is not only involved in stress adaptation but also in growth phase-dependent gene expression [17, 18]. Moreover, the transcription profile of the C. glutamicum sigB gene is very similar to that of the orthologous sigB gene of M. tuberculosis [9] and to the expression pattern of the rpoS gene encoding the alternative sigma factor σS of E. coli [35]. In all cases, transcription of the gene was maximal during transition from exponential to stationary phase as well as under certain environmental stress conditions [2, 36]. For C. glutamicum, Oguiza et al. analyzed the abundance of sigA and sigB transcripts during growth in complex medium by Northern hybridization and found out that both transcripts were abundant during exponential growth phase and abundance decreased simultaneously in stationary phase. During early exponential phase, the sigA transcript was more abundant than the sigB transcript [20].

Transition from exponential to stationary growth phase changed the transcription profile of C. glutamicum

Comparative DNA microarray analyses between the sigB-proficient and sigB-deficient C. glutamicum strain delivered a genome-wide view on relative transcript abundances during transition phase. Quite a large number of genes identified here falls into three functional classes. They encode either carbon metabolism or transport, stress defence and membrane processes. Weber et al. identified several hundred genes as to be controlled by the non-essential sigma factor σS in E. coli which is also higher expressed during transition phase. A large number of the respective proteins with known or predicted functions fall into similar classes as in our study. These are protein-processing reactions, stress-defence mechanisms, membrane processes and regulatory functions [8]. It can be assumed that E. coli SigS as well as C. glutamicum SigB have similar functions as main regulators of cellular functions at suboptimal growth, e.g. the scavenging of various nutrients and increased resistance against various toxic compounds. The genes that are regulated by the putative SigB-ortholog in S. coelicolor also belong to similar functional complexes. Especially, a large number of genes encoding membrane-associated, secreted and cell-wall-related proteins are transcribed with the help of SigB, suggesting the involvement in protection against oxidative damage and osmotic stress [37].

Reduced transcription of genes under conditions of an enhanced expression of sigB may occur through a competition for the core polymerase between SigA and SigB. Because of this competition, the expression of the sigA gene also decreases in the transition phase since the sigA gene is apparently transcribed with the help of SigA [19]. The genes negatively affected by the presence of SigB might therefore be transcribed predominantly with the help of SigA in C. glutamicum. Studies in E. coli demonstrated that the affinity of σS for the core RNA polymerase is lower than that of σ70 [38, 39], and since the amount of RNA polymerase is limiting, there is a competition between both sigma factors for binding to the core enzyme during transition phase [40]. The competitiveness of a given sigma factor for the core RNA polymerase is determined by its abundance in the cell and its relative affinity for the RNA polymerase [41]. Therefore, a concomitant decrease in abundance of SigA and an increase of SigB in C. glutamicum during transition phase should support the interaction of SigB with the RNA polymerase core enzyme and should lead to a high level expression of certain genes, fulfilling a vital role in this phase and later stages of growth.

Conclusion

In this study, we demonstrated that SigB is involved in gene regulation at the transition from exponential to stationary growth phase. During transition phase, the sigB gene showed an enhanced expression, while simultaneously sigA mRNA decreased in abundance. This might cause a replacement of SigA by SigB at the RNA polymerase core enzyme and in turn results in increased expression of genes relevant for transition phase of growth, either to cope with nutrient limitation or with the accompanying oxidative stress. The increased expression of genes encoding anti-oxidative or protection functions also prepares the cell for upcoming limitations and environmental stresses. In this functional role the C. glutamicum SigB is similar to RpoS of E. coli. However, this study has only addressed a single functionality of SigB and other physiological roles, especially with respect to certain environmental stresses might exist. These functional complexes as well as the potential regulation of the sigB gene and its encoded protein by other transcriptional regulators or by anti-sigma factors are interesting subjects of future studies.

Methods

Bacterial strains and growth conditions

E. coli was routinely grown at 37°C in Luria-Bertani medium [42] supplemented with 2 g/l glucose (LBG). C. glutamicum strains were grown at 30°C in minimal medium MM1 (MMYE without yeast extract) [43]. For batch cultures, 100 ml of stationary shake-flask cultures of C. glutamicum was used to inoculate a 7-l fermentor (MBB, Büchi, Switzerland) containing 5 l minimal medium MM1. The cultures were grown at 30°C with a pO2 level of 30%. The pH set point was 7, regulated with 2 M NaOH and 10% (w/v) H3PO4. Glucose was limited (25 g/l) to induce the stationary phase by glucose exhaustion.

DNA and PCR techniques

E. coli DH5αMCR [44] was used for cloning experiments. Vector DNA was prepared from E. coli cells by alkaline lysis using the QIAprep Spin Miniprep Kit (Qiagen, Hilden, Germany). DNA restriction fragments required for cloning were purified from agarose gels by means of the QIAEX II Gel Extraction Kit (Qiagen). All recombinant DNA techniques followed standard procedures [42]. E. coli and C. glutamicum cells were transformed by electroporation [45, 46]. Chromosomal DNA of C. glutamicum was prepared as described earlier [47].

PCR experiments were carried out with a PTC-100 thermocycler from MJ Research (Watertown, MA) and Pfu DNA polymerase. Initial denaturation was conducted at 94°C for 2 min followed by denaturation for 30 s, annealing for 30 s at a primer-dependent temperature, and extension at 72°C for 45 s. This cycle was repeated 30 times, followed by a final extension step at 72°C for 3 min. PCR products were purified by using the QIAquick PCR Purification Kit (Qiagen). Cloning of PCR products was performed in E. coli TOP10 by means of the Zero Blunt TOPO PCR Cloning Kit (Invitrogen, Karlsruhe, Germany).

Construction of the sigB deletion mutant C. glutamicum CL1

A defined chromosomal deletion within the sigB gene of C. glutamicum RES167 [46] was constructed with the pK18 mobsacB vector system which helps to identify an allelic exchange by homologous recombination [48]. The respective plasmid (pCL1) was constructed by the gene SOEing technique [49]. Gene replacement in the chromosome of C. glutamicum RES167 was verified by PCR experiments.

Total RNA isolation from C. glutamicum cells for DNA microarray hybridization

C. glutamicum cells were harvested during exponential, transition and stationary phase, as described previously [23]. Isolation of RNA was carried out by means of the RNeasy Mini Kit (Qiagen) following the manufacturer's instructions. The RNase-Free DNase set (Qiagen) was applied for on-column removal of DNA. A second DNase I digestion was performed by using the DNase I Kit (Sigma-Aldrich, Taufkirchen, Germany).

The C. glutamicum DNA microarray used in this study was developed by Hüser et al. [23]. Synthesis and labeling of cDNA as well as DNA microarray hybridization, signal detection and data analysis followed protocols described previously [23]. Monitoring of gene expression was performed with two biological replicates. Technical replicates were analyzed by using label-swapping, resulting in a total number of four measurements.

Real-time RT-PCR assays

RT-PCR experiments were performed with the LightCycler instrument (Roche Diagnostics), using the QuantiTect SYBR Green RT-PCR Kit (Qiagen). Analyses were carried out with 1 μg of total RNA as template and the following cycler program: reverse transcription for 30 min at 45°C, initial activation for 15 min at 95°C and 3-step-cycling with denaturation for 10 s at 94°C, annealing for 40 s at 56°C and extension for 180 s at 68°C. Differences in gene expression were determined by comparing the crossing points of two samples measured in eight replicates. The crossing points were calculated by the LightCycler software version 3 (Roche Diagnostics).

RACE-PCR assay for the identification of transcriptional start sites

Total RNA of C. glutamicum RES167 grown in MM1 medium was used for the determination of transcriptional start sites by means of the 5' RACE Kit (Roche Diagnostics). RACE PCR was carried out as recommended by the supplier, using 2 μg of total RNA. Resulting PCR products were ligated into the vector pCR2.1 by applying the TOPO TA cloning system and chemically competent E. coli TOP10 cells (Invitrogen). Sequencing of RACE products was carried out by IIT Biotech (Bielefeld, Germany).

Declarations

Acknowledgements

We thank M. Scheidle, T. Schäffer and Prof. Dr. E. Flaschel (Department of Fermentation Technology, Bielefeld University) for advice in microbial fermentation techniques. The financial support from Degussa AG (Düsseldorf, Germany) is also acknowledged.

Authors’ Affiliations

(1)
Institut für Genomforschung, Centrum für Biotechnologie, Universität Bielefeld

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