• We are sorry, but NCBI web applications do not support your browser and may not function properly. More information
Logo of narLink to Publisher's site
Nucleic Acids Res. Apr 2011; 39(7): 2931–2942.
Published online Nov 23, 2010. doi:  10.1093/nar/gkq1177
PMCID: PMC3074128

Structures of carbon catabolite protein A–(HPr-Ser46-P) bound to diverse catabolite response element sites reveal the basis for high-affinity binding to degenerate DNA operators

Abstract

In Gram-positive bacteria, carbon catabolite protein A (CcpA) is the master regulator of carbon catabolite control, which ensures optimal energy usage under diverse conditions. Unlike other LacI-GalR proteins, CcpA is activated for DNA binding by first forming a complex with the phosphoprotein HPr-Ser46-P. Bacillus subtilis CcpA functions as both a transcription repressor and activator and binds to more than 50 operators called catabolite response elements (cres). These sites are highly degenerate with the consensus, WTGNNARCGNWWWCAW. How CcpA–(HPr-Ser46-P) binds such diverse sequences is unclear. To gain insight into this question, we solved the structures of the CcpA–(HPr-Ser46-P) complex bound to three different operators, the synthetic (syn) cre, ackA2 cre and gntR-down cre. Strikingly, the structures show that the CcpA-bound operators display different bend angles, ranging from 31° to 56°. These differences are accommodated by a flexible linkage between the CcpA helix-turn-helix-loop-helix motif and hinge helices, which allows independent docking of these DNA-binding modules. This flexibility coupled with an abundance of non-polar residues capable of non-specific nucleobase interactions permits CcpA–(HPr-Ser46-P) to bind diverse operators. Indeed, biochemical data show that CcpA–(HPr-Ser46-P) binds the three cre sites with similar affinities. Thus, the data reveal properties that license this protein to function as a global transcription regulator.

INTRODUCTION

Bacteria use carbon sources in a hierarchical manner, which ensures that the energy source most beneficial for survival is utilized preferentially. This mechanism, called carbon catabolite control, is primarily carried out at the level of transcription (1–6). In Gram-positive bacteria, carbon catabolite control is mediated in large part by the carbon catabolite protein A (CcpA), a global transcriptional regulator (7). CcpA is a member of the LacI-GalR family of transcription regulators, which are characterized by the presence of an N-terminal, approximately 60 residue DNA-binding domain and a larger effector binding, oligomerization C-terminal domain (C-domain) (8–14). Small molecules, either inducers or corepressors, bind in a cavity between two sub-domains that comprise the C-domain to regulate DNA binding (9–10,12–14). These small molecules lock the C-domain into either a closed or open conformational state. In the closed state, interactions between the DNA-binding hinge regions are stabilized allowing them to fold in the presence of cognate DNA to form the DNA binding ‘hinge helices’ (9–10). The finding that mutants unable to produce fructose-1,6-bisphosphate do not exhibit carbon catabolite control, led to the discovery that instead of a small molecule, CcpA binds a protein as its effector. Specifically, CcpA binds the Ser46 phosphorylated form of histidine-containing phosphocarrier protein (HPr) (15). HPr is the energy coupling protein of the phosphoenolpyruvate-dependent carbohydrate:phosphotransferase system (PTS), which transports selected carbohydrates into the cell. But in the presence of high concentrations of glucose, HPr is phosphorylated on Ser46, allowing the phosphoprotein to bind CcpA and exert carbon catabolite control (15–20). The structure of a B. megaterium CcpA–(HPr-Ser46-P)-catabolite response element (cre) complex revealed that although HPr-Ser46-P binds to a region of CcpA > 30 Å from the DNA, this phosphoprotein stabilizes the closed state of the CcpA C-domains and induces relocation of key residues located at the interface of the DNA-binding and C-domains. The ultimate outcome is a juxtaposition of the CcpA DNA-binding domains that allows the 2-fold-related hinge helices to fold in the presence of cognate DNA and make key minor groove interactions at a conserved CpG step as well as positioning the helix-turn-helix (HTH) motif for major groove binding (11).

In Bacillus subtilis, carbon catabolite control by CcpA has been studied extensively and the data indicate that ~10% of the genome responds directly or indirectly to CcpA, underscoring its vital metabolic role (21). The multiple genes regulated by CcpA encode proteins involved in carbon metabolism and utilization, including enzymes, transporters and transcription factors (21). To carry out this regulation, CcpA acts as both a repressor and an activator. The genes activated by CcpA include ackA and pta, which are involved in the formation of acetate. CcpA–(HPr-Ser46-P) also triggers expression of the ilv-leu operon, which is involved in the biosynthesis of branched chain amino acids. Genes that are directly repressed by CcpA include those involved in carbon, nitrogen and phosphate metabolism (4–6). Thus, CcpA plays a central role in the coordinated regulation of catabolism and anabolism to ensure optimal cell growth under varying environmental conditions. To carry out its global role as a transcription regulator, CcpA–(HPr-Ser46-P) binds to a number of diverse cre sites in target promoters and genes. Interestingly, the location of cre site(s) within each promoter varies and correlates with whether CcpA functions as a repressor or an activator (4). For example, promoters with upstream cre sites such as ackA and pta appear to be primarily activated by CcpA (22–25). In contrast, promoters with overlapping cre sites such as amyE, bglP, ccA, cdtP, glpF, phoP and acuA are repressed (26–32). When bound at these locations, CcpA–(HPr-Ser46-P) apparently interferes with binding of the transcription machinery. By binding to cre sites located far downstream of the transcription initiation site, such as in the case of the gnt operon, CcpA–(HPr-Ser46-P) functions as a roadblock, again leading to transcription repression (4, 33). However, there may be exceptions in these location specific effects. For instance, CcpA–(HPr-Ser46-P) binding upstream of the promoter in the levanase operon appears to prevent transcription (34).

cre sites are highly degenerate pseudo-palindromes with the consensus sequence, W1T2G3N4N5A6R7C8G9N10W11W12W13C14A15W16 (where W stands for A or T, R for A or G and N for any base) (4,35,36). The lack of stringent sequence conservation in the in vivo cre sites suggests that CcpA–(HPr-Ser46-P) can bind sites with a high degree of plasticity. Consistent with this, examination of the experimentally verified cre sites reveals that the central CpG step and the G-C base pair at position 3 are the only completely conserved nucleotides. How CcpA binds such a diverse set of operator sites and the affinity with which CcpA binds these sites is unknown. To gain insight into these questions we carried out binding studies on B. subtilis CcpA–(HPr-Ser46-P) and three distinct cre sites; the synthetic (syn) cre, ackA2 cre and gntR-down cre and determined the structures of these complexes by X-ray crystallography.

MATERIALS AND METHODS

Purification of B. subtilis CcpA and HPr-Ser46-P

The B. subtilis ccpA gene, fused to a C-terminal hexa-histidine (His6)-tag encoding sequence, was subcloned via XbaI/BamHI into pET3c (Novagen) producing pWH653 (Table 1) (37). BL21(DE3) cells were transformed with the pWH653 expression vector and protein expression was induced by the addition of IPTG to a final concentration of 1 mM. The resulting cells were suspended in buffer A (20 mM Tris–HCl, pH 7.5, 300 mM NaCl, 10 mM imidazole, pH 8.0) and incubated with 5 µg/ml protease inhibitor cocktail tablets (Roche) for 20 min. After cell disruption via microfluidizer the supernatant was loaded onto a Ni2+-NTA column and the protein purified using a step gradient between buffer A and buffer B (20 mM Tris–HCl, pH 7.5, 300 mM NaCl, 500 mM imidazole, pH 8.0). CcpA-containing fractions were pooled and concentrated in the presence of 5% glycerol. The protein was purified further using size exclusion chromatography (S200 column) in buffer C (20 mM Hepes, pH 7.5, 150 mM NaCl, 3 mM EDTA, 5% glycerol).

Table 1.
Strains and plasmids

Bacillus subtilis HPr was expressed in Escherichia coli FT1/pLysS/pWH466 as previously described (37). Cells containing the expressed protein were suspended in buffer D (10 mM Tris–HCl, pH 7.5) and incubated with 5 µg/ml RNase, 10 µg/ml DNase and protease inhibitor cocktail tablets (Roche) for 20 min. After cell disruption the lysate was heated to 70°C and centrifuged at 20 000 rpm for 60 min. The partially purified HPr from the supernatant was phosphorylated using HPr kinase as described previously (19). The resulting phosphorylated protein, HPr-Ser46-P, was subjected to anion exchange chromatography on a Sepharose QFF column using a linear gradient between buffer D and buffer E (10 mM Tris–HCl, pH 7.5, 1 M NaCl). HPr-Ser46-P containing fractions were pooled and concentrated using an Amicon Ultra 3 kDa filter. A final purification step was performed using an S75 column (GE Healthcare). For the surface plasmon resonance (SPR) measurements glycerol free HBSE buffer (150 mM NaCl, 3 mM EDTA, 10 mM Hepes, pH 7.4) was used as storage buffer for both proteins since glycerol can affect the measurements.

Determination of DNA-binding affinities via fluorescence polarization

The binding affinities of CcpA for the syn cre (5′-CTGTTAGCGCTTTCAG-3′), ackA2 cre (5′-TTGTAAGCGTTATCAA-3′) and gntR-down cre (5′-TTGAAAGCGGTACCAT-3′) were determined by fluorescence polarization (FP) at 25°C using a Beacon 2000 fluorescence polarization instrument (38). 5′-Fluorescein labelled hairpin cre elements, where the complementary 16 bp of the syn cre, ackA2 cre and gntR-down cre, were separated by a loop consisting of five cytosines, were used. For each measurement CcpA was titrated into a 1-ml reaction cell containing a buffer consisting of 150 mM NaCl, 20 mM Hepes, pH 7.4, 3 mM EDTA, 10 µg/ml poly(dIdC) and 1 nM 5′-fluorescein-labelled oligonucleotide in the presence and absence of 50 µM HPr-Ser46-P. All measurements were performed in triplicate.

Determination of DNA-binding affinities via SPR

SPR measurements were performed on a Biacore X instrument operated at 25°C (Biacore, Uppsala, Sweden). The coupling of the DNA and the measurement was carried out as described previously (39). The DNA sites used are shown in Table 2. HBS–EP buffer purchased from Biacore was used at a flow rate of 40 µl/min for all measurements since mass transport was minimal. The running buffer and each sample were supplemented with 50 µM HPr-Ser46-P during the kinetic experiments to minimize bulk effects. To ensure full saturation of the gntR-down cre with the protein complex, 75 µM HPr-Ser46-P was used. Titrations were carried out with 5 or 20 to 100 nM CcpA(His)6. To regenerate the chip and to stop the dissociation of the CcpA–(HPr-Ser46-P)-complex from the chip, 80 µl pure HBS-EP were injected at 40 µl/min after each sample.

Table 2.
Oligonucleotides

Crystallization of CcpA–(HP-Ser46-P) bound to the syn, ackA2 and gntR-down cre sites

The B. subtilis CcpA–(HPr-Ser46-P) complex was crystallized in the presence of cre elements used in the binding studies: the syn cre (5′-CTGTTAGCGCTTTCAG-3′), ackA2 cre (5′-TTGTAAGCGTTATCAA-3′) or gntR-down cre (5′-TTGAAAGCGGTACCAT-3′). Each CcpA–(HPr-Ser46-P)–DNA complex (using a 1:2:1 ratio of CcpA dimer: HPr-Ser46-P monomer: DNA duplex) was mixed with various reservoir solutions and crystallized using the hanging drop vapor diffusion method. Notably, different conditions were required to obtain each of the crystals. Crystals of the CcpA–(HPr-Ser46-P)–syn cre were obtained by mixing the complex 1:1 (v:v) with a reservoir of 20% PEG 3350 and 0.2 M ammonium formate. Crystals of the CcpA–(HPr-Ser46-P)–ackA2 complex were grown by mixing the complex 1:1 with a reservoir of 17.5% PEG 8000, 0.2 M ammonium sulphate, 0.01 M magnesium chloride, 0.05 M MES pH 5.6. Crystals of the CcpA–(HPr-Ser46-P)–gntR-down cre complex were produced by mixing the complex 1:1 with a reservoir of 20% PEG 6000, 0.1 M citric acid, pH 5.0. Despite the different requirements for obtaining the crystals, all three took the space group P212121. The crystals were cryoprotected for data collection by supplementing the reservoirs with 25%, 25% and 20% glycerol, respectively, and dipping each crystal for several seconds in the cryoprotectant before looping and placing in the cryostream. X-ray intensity data were collected at the Advanced Light Sources (ALS, Berkeley, CA, USA) beamline 8.2.1 (Table 3).

Table 3.
Selected crystallographic data for CcpA-(HPr-Ser46-P)-DNA structures

Structure determination and refinement

All three structures were solved by molecular replacement with MolRep using the same starting model, 2FEP [the B. subtilis CcpA (residues 60–334)–(HPr-Ser46-P) structure] (11,40). After rigid-body refinement in CNS, clear electron density for the DNA-binding region, residues 1–59, and the DNA was revealed. The cre sites and DNA-binding residues 2–59 were then built into their respective densities and positional (xyz) refinement was carried out. The 5′–3′ directions of the DNA sites were ascertained by examination of the electron density and Rfree. After several rounds of refinement and extensive rebuilding, xyz and thermal parameter (B factor) refinement was utilized for the CcpA–(HPr-Ser46-P)–ackA2 and CcpA–(HPr-Ser46-P)–syn structures (41,42). The final CcpA–(HPr-Ser46-P)–ackA2 structure includes all 32 nt of the DNA duplex, residues 2–333 of each CcpA subunit, residues 2–88 of each HPr-Ser46-P molecule, four sulphate molecules and 46 solvent molecules. The final CcpA–(HPr-Ser46-P)–syn structure includes all nucleotides of the DNA duplex, residues 2–333 of each CcpA subunit, residues 2–88 of each HPr-Ser46-P molecule and 49 solvent molecules. The final CcpA–(HPr-Ser46-P)–gntR-down structure includes all nucleotides of the DNA duplex, residues 2–333 of each CcpA subunit and residues 2–88 of each HPr-Ser46-P molecule. Selected data collection and refinement statistics are given in Table 3.

RESULTS AND DISCUSSION

CcpA–(HPr-Ser46-P) binding to the syn, ackA2 and gntR-down cre sites

Bacillus subtilis CcpA–(HPr-Ser46-P) has been shown to bind to a number of diverse cre operators, however, there is no information regarding its relative binding affinities for these sites. Hence, we began our study by determining the equilibrium binding constants (Kd’s) of CcpA–(HPr-Ser46-P) for three well-studied cre sites, the synthetic (syn) cre, ackA2 cre and the gntR-down cre (Figure 1A). The syn cre is an artificial operator that binds the B. megaterium CcpA–(HPr-Ser46-P) complex with high affinity and was used in structure determination of the B. megaterium CcpA–(HPr-Ser46-P)–DNA complex (11). Given that B. megaterium and B. subtilis CcpA proteins share 76% sequence identity, we hypothesized that the B. subtilis CcpA–(HPr-Ser46-P) complex would also bind the syn cre with high affinity. Indeed, using a fluorescence polarization (FP)-based DNA-binding assay, we determined that B. subtilis CcpA–(HPr-Ser46-P) bound the 16-bp syn cre (5′-CTGTTAGCGCTTTCAG-3′) with a Kd of 10 ± 1 nM (Figure 1B). As has been shown previously, high-affinity binding to cre DNA requires HPr-Ser46-P. In accord, in the absence of HPr-Ser46-P, CcpA bound the syn cre with 100-fold reduced affinity (Kd = 1020 ± 110 nM) (Supplementary Figure S1A).

Figure 1.
CcpA–(HPr-Ser46-P)–cre site promiscuity. (A) Sequences of the three cre sites, syn, ackA2 and gntR-down, used in the study. Asterisks over the sequences show the locations where the sites differ. Below the three sites used in the study ...

The ackA2 cre is one of two cre sites in the promoter of the gene encoding acetate kinase (31). ackA2 and the second cre site, called ackA1, are centered at 22 and 82 bp, respectively, upstream of the 35 box and differ from each other in four positions in the right-half site of the operator (ackA1: 5′-TTGTAAGCGTTCATCA-3′, ackA2; 5′-TTGTAAGCGTTATCAA-3′). However, only the ackA2 cre plays a role for CcpA-dependent carbon catabolite activation of ackA, while the ackA1 cre is not required (31). The ackA2 cre differs from the syn cre in 5 nt positions (Figure 1A), yet CcpA–(HPr-Ser46-P) bound the ackA2 cre with essentially the same affinity (Kd, 6.4 ± 1 nM, Figure 1B). Again, the absence of HPr-Ser46-P resulted in a significant, >100-fold reduction in binding with a Kd = 950 ± 90 nM (Supplementary Figure S1B).

Similar to ackA, the gntR operon is regulated by two putative cre sites. However, in this case one site, gntR-down is located within a gene, specifically, the first gene of the gnt operon. The second putative cre, gntR-up is located in the promoter region. While gntR-down was shown to be bound by CcpA–(HPr-Ser46-P), gntR-up showed no interaction with the complex, as ascertained by DNase I protection studies (43). The gntR-down cre diverges from the syn cre in seven of 16 positions and four of 16 positions when compared to the ackA2 cre (Figure 1A). But again, binding studies demonstrated that CcpA–(HPr-Ser46-P) bound this site with essentially the same Kd, 5.2 ± 0.2 nM, as the syn and ackA2 cre sites (Figure 1B). Moreover, this binding was dependent on HPr-Ser46-P as the Kd of CcpA alone for this site was 900 ± 60 nM (Supplementary Figure S1C).

Given the significant differences in the sequences of the syn, ackA2 and gntR-down sites, the finding that CcpA–(HPr-Ser46-P) bound these sites with the same Kd was surprising. Thus, we determined Kd’s from the rate constants of CcpA–(HPr-Ser46-P) binding to the ackA2 cre, syn cre and gntR-down cre using SPR. For these studies, 4000 RU (Response Units) of Neutravidin, a streptavidin analogue, were coupled to a CM5-chip. Subsequently, 5′ biotinylated cre-DNA was coupled in flowcell 2 and 5′ biotinylated reference DNA was in flowcell 1. As reported previously, 50 µM HPr-Ser46-P was contained in the running buffer to observe only the dissociation of the CcpA–(HPr-Ser46-P) complex from the DNA (39). The kinetics were analysed via titration of 5 or 20 to 100 nM CcpA and 50 µM HPr-Ser46-P (Supplementary Data). All data were fitted with the BIAEVALUATION software 3.1 to calculate the association and dissociation rate constants from the sensorgrams. Representative sensorgrams with the calculated best fits are shown in Figure 2 and the resulting rate constants are given in Table 4. The binding constants were highly congruent with those obtained by FP studies. Specifically, the Kd’s for CcpA–(HPr-Ser46-P) binding to the syn, ackA2 and gntR-down cre sites were 3.8 ± 0.1, 1.6 ± 0.4, 3.0 ± 0.4 nM, respectively (Figure 2). Thus, only small differences in the Kd’s were observed between the two studies, likely due to different buffer conditions and oligodeoxynucleotide lengths. However, the critical finding is that both studies demonstrate that CcpA–(HPr-Ser46-P) complex binds the three diverse cre sites with essentially the same affinity. To understand the molecular mechanisms by which CcpA–(HPr-Ser46-P) can interact with high affinity to such divergent cre sequences we determined crystal structures of the three complexes.

Figure 2.
SPR analysis of CcpA–(HPr-Ser46-P) binding to cre elements reveals similar association and dissociation rates. The titrations were carried out with 5 or 20 to 100 nM CcpA. To reduce bulk effects, the running buffer was supplemented with ...
Table 4.
Association and dissociation rate constants and equilibrium binding constants of the CcpA–(HPr-Ser46-P) complex for cre sites

Structure determination of B. subtilis CcpA–(HPr-Ser46-P)–cre complexes

For structural studies, we crystallized CcpA–(HPr-Ser46-P) with 16-bp oligodeoxynucleotides containing the three different cre sites used in the FP-binding studies; the syn cre (5′-CTGTTAGCGCTTTCAG-3′), the ackA2 cre (5′-TTGTAAGCGTTATCAA-3′) and the gntR-down cre (5′-TTGAAAGCGGTACCAT-3′). The DNA sites were designed to be the same length in hopes that the crystals would adopt similar packing environments, thus permitting a direct comparison of the structures. Interestingly, different conditions were required to produce each crystal. However, the crystals all took the orthorhombic space group, P212121, and had very similar cell edges and crystal packing. The CcpA–(HPr-Ser46-P)–syn, CcpA–(HPr-Ser46-P)–ackA2 and CcpA–(HPr-Ser46-P)–gntR-down structures were solved and refined to Rwork/Rfree values of 21.2%/26.9%, 21.7%/27.2% and 22.1%/27.6% to 2.97 Å, 2.95 Å and 3.30 Å, respectively (Table 3; ‘Materials and Methods’ section). Each structure contains a CcpA dimer, two HPr-Ser46-P molecules and an entire DNA duplex in the crystallographic asymmetric unit (ASU). The presence of an entire dimer bound to a DNA duplex in the ASU allowed an unfettered comparison of the structures, as there is no 2-fold disorder in the DNA or protein to complicate our structure analyses.

Overall structures of CcpA–(HPr-Ser46-P)–cre complexes

The overall structures of the CcpA–(HPr-Ser46-P)–cre complexes show that HPr-Ser46-P binds the surface of CcpA with a stoichiometry of one HPr-Ser46-P molecule per CcpA subunit, as previously observed in the B. megaterium CcpA–(HPr-Ser46-P)–cre structure (Figure 3) (11). The three B. subtilis CcpA–(HPr-Ser46-P) complexes can be superimposed onto the B. megaterium CcpA–(HPr-Ser46-P) complex with root mean square deviations (RMSDs) ranging from 2.4 Å to 2.6 Å for all Cα atoms, including both CcpA subunits and both HPr-Ser46-P molecules (Supplementary Figure S2). Like B. megaterium CcpA and other LacI-GalR family members, B. subtilis CcpA is composed of an N-terminal DNA-binding domain (residues 1–59) and a C-terminal dimerization/HPr-Ser46-P-binding domain (residues 60–334) (7–12). The DNA-binding domain has two distinct DNA-binding elements or modules; a three-helix bundle, herein referred to as the helix-turn-helix-loop-helix (HTHLH), where helices 1 and 2 form the major groove binding helix-turn-helix motif (HTH) (helix 1: residues 5–12, helix 2: residues 16–24, helix 3: residues 31–44) and the hinge helix, helix 4 (residues 50–58), which inserts into the minor groove of the central CpG step, thereby kinking the DNA (Figure 3). The CcpA C-domain can be divided into two structurally similar subdomains, the N-subdomain and the C-subdomain. The N-subdomain consists of a six-stranded parallel β-sheet, surrounded by four α-helices. The C-sub-domain contains a five β-stranded parallel sheet and five surrounding α-helices. The subdomains are connected by three crossovers that can act as a joint to permit rotation of the two subdomains. The CcpA dimerization interface is extensive and buries 3900 Å2 surface area from solvent.

Figure 3.
Structures of CcpA–(HPr-Ser46-P) bound to three cre sites. Shown from left to right are the ribbon diagrams of the CcpA–(HPr-Ser46-P)–syn, CcpA–(HPr-Ser46-P)–ackA2 and CcpA–(HPr-Ser46-P)–gntR-down ...

CcpA–(HPr-Ser46-P)–cre structures: plasticity in DNA binding

The three CcpA–(HPr-Ser46-P)–cre complexes are similar in overall structure and arrangement, however, there are some notable differences (Figures 3 and and4A).4A). In particular, an analysis of the DNA structure using Curves+ (44) reveals that whilst the syn cre site is bent by 31° when bound by CcpA–(HPr-Ser46-P), the ackA2 and gntR-down cre sites are bent by 56° and 41°, respectively (Figure 4B and C). In addition, the syn cre DNA minor groove has a greater width, 13.1 Å, than either of those of the ackA2 and gntR-down cres, which have minor groove widths of 12.3 Å and 12.4 Å, respectively. Consistent with the differences in DNA structural distortions, the CcpA DNA-binding domains display differences in their relative conformations. This is readily observed in superimpositions, which show that whilst the overlay of CcpA residues 50–330, which contains the hinge helices and C-domains, results in rmsds between 0.3 Å and 0.4 Å, inclusion of residues 2–49 results in RMSDs of 0.9 Å and 1.0 Å when comparing subunits from the CcpA–(HPr-Ser46-P)–syn structure to those from the CcpA–(HPr-Ser46-P)–ackA2 and CcpA–(HPr-Se46-P)–gntR-down structures, respectively. In contrast, the superimposition of residues 2–330 of the ackA2 and gntR-down CcpA subunit structures results in an rmsd of only 0.45 Å, which is within the experimental error of the coordinates (~0.50 Å from the Luzzati plot analysis). These comparisons indicate that the HTHLH DNA-binding module, residues 2–49, of the syn bound structure displays an altered conformation relative to the corresponding HTHLH modules from the ackA2 and gntR-down bound structures (Figure 4A). This difference involves a rigid-body movement of the HTHLH unit because superimpositions of the individual HTHLH units show that they are essentially identical in all three structures (the HTHLH motifs can be superimposed with rmsds of 0.3–0.4 Å). The HTHLH of both subunits of the syn bound structure undergo the same relative shift (Figure 4A). The flexible attachment by residues 45–50 of the HTHLH unit to the hinge helices appears important in permitting this rigid-body movement and requires the ability of residues 45–50 to take multiple conformations. Such an ability to rotate allows the HTHLH modules to adjust to different DNA conformations and hence allows optimal docking of the HTH units onto the DNA major groove (Figure 4A).

Figure 4.
CcpA–(HPr-Ser46-P)–cre binding requires protein and DNA flexibility. Different orientations of the HTHLH modules and the DNA conformations of CcpA–(HPr-Ser46-P) bound cre sites. (A) View of the DNA-binding HTHLH modules and cognate ...

Interestingly, there are no data that would suggest why the sequences of the ackA2 and gntR-down cre sites would display larger bend angles compared to the syn sequence (45). The smaller overall bend in the syn bound site appears necessary for permitting the specific interaction of the HTH motif, which is located closer to the centre of the this cre site. Thus, it is not clear whether the altered DNA structures are the result of bend angle predispositions or are the outcome of the insertion of the CcpA–hinge helices into the central CpG step of each sequence. Regardless of the underlying cause, our structures demonstrate that CcpA is able to adjust to significant changes in DNA conformation by the inherent flexibility exhibited by the linker between its two independent DNA-binding modules, the HTHLH and hinge helices.

Flexibility between DNA-binding modules allows optimal docking

The above analysis demonstrates that CcpA can adjust to different DNA distortions because of the modularity and flexibility of its two DNA-binding elements. But this does not explain how CcpA can interact specifically with the DNA nucleobases of such diverse DNA sequences. A detailed comparison of the contacts made by CcpA to each cre site shows only two conserved side chain–base interactions that appear specific. These are the major groove contacts from HTH residue Arg22 to Gua3 (two guanidinium side chain hydrogen bonds to the O6 and N7 atoms of Gua3) and hinge-helix residue Leu56 to the CpG step in the DNA-minor groove (Figure 5). These two interactions precisely anchor or dock the HTHLH and the hinge helix onto the major and minor grooves of the cre DNA site, respectively. While the Arg22 to guanine contact is a ‘standard’ type of specificity determining interaction that has been observed in multiple protein–DNA complexes, the Leu56–hinge helix interaction with the highly rolled central CpG step (roll angles range from 44° to 45°) is unusual (Figure 5A and B). The formation of this interaction is likely a multistep, complex process, as it requires the coupling of DNA distortion with hinge helix folding and leucine insertion into the minor groove. In the CcpA apo state, the hinge region exists in an unfolded state (11). Hence, to form the interaction, the hinge helices must form and the folding is likely coupled to CpG distortion. Interestingly, in all the structures, hinge helix backbone atoms make weak (non ideal geometry) but specific hydrogen bonds to the nucleobases of the central CpG step; the carbonyl oxygen of Ala53 and the amide nitrogen of Ala57, interact with the Gua N2 and Cyt O2 atoms, respectively (range of hydrogen bond distances in the three structures are; Gua(N2)-Ala53(C = O): 3.1 Å to 3.4 Å and Cyt(O2)-Ala57(NH2): 3.1 Å to 3.6 Å) (Figure 5B). These contacts would favour coupled helix folding with DNA distortion and also impart a preference for a CpG step. Finally, hinge helix folding precisely orients the 2-fold-related Leu56 residues to insert into the widened minor groove. The perfect fit of the Leu56 residues into this space provides side chain specificity (Figure 5B). Indeed, this leucine is completely conserved in all CcpA proteins and all characterized LacI-GalR proteins that utilize hinge helices to bind DNA (9,11,14).

Figure 5.
CcpA–cre interactions. (A) Close up view of the Arg22 interaction with Gua3 and the van der Waals contact between the side chain Cβ of Asn29 with Thy2 (indicated by double headed arrow). Also note the stacking of the Arg22 side chain with ...

As would be expected if they play essential roles in DNA binding, Arg22 and Leu56 are conserved in all CcpA proteins (11). Moreover, Gua3, its 2-fold-related counterpart, and the central CpG step are the only completely conserved bases amongst the more than 50 identified B. subtilis cre sequences. Studies have demonstrated that these two base pairs are essential for transcription regulation by CcpA (Figure 1A) (4,35). In particular, Weickert and Chambliss carried out a detailed analysis on the affect of site-directed mutagenesis of the cre site on catabolite repression of the B. subtilis amylase operon (35). Their studies underscored the significant flexibility in the operator sequence and revealed the consensus, TG3WA*ANC8G9NTNWC14A (where bolded letters represents the most critical bases and the A* indicates the transcription start site) (35). Thus, aside from the conserved guanine/cytosine base pairs at positions 3/14 and 8/9, the only other position that shows a strong preference for specific nucleotides are Thy2 and its 2-fold-related nucleotide, Ade15 (Figure 1A). Our current structures show that the methyl groups of Thy2A (and Thy15B) are contacted by the Cβ atom of residue Asn29 from each subunit. Asn29 is completely conserved amongst CcpA proteins. Interestingly, the corresponding Asn-CβThy2 contact was not observed in the B. megaterium CcpA–(HPr-Ser46-P)–DNA structure, suggesting that it cannot be a CcpA specificity determining contact (11). However, Thy2 in both the B. subtilis and B. megaterium CcpA–(HPr-Ser46-P)–DNA structures contain an unusual stacking interaction with the arginine (Arg22 in B. subtilis and Arg21 in B. megaterium), which makes specific hydrogen bonds with the guanines at positions 3 and 14 (Figure 5A and C). This stacking/van der Waals interaction between the arginine side chain and the thymine base fits the criteria for what has been termed a 5′-pyrimidine-guanine-3′ (5′-YpG-3′) interaction (46,47). This interaction is thought to arise because of the inherent flexibility of pyridimine-guanine steps, which allows them to become unstacked more readily (48). In a 5′-YpG-3′interaction, the arginine side chain makes specific hydrogen bonds to the major groove face of the 5′-guanine nucleobase, whilst simultaneously contacting the unstacked preceding pyrimidine (48). This type of recognition mode was initially shown to be critical for the specific DNA binding of the Saccharomyces cerevisiae sporulation specific transcription factor, Ndt80, to the middle sporulation element (MSE) DNA site (46). A subsequent survey by the Glover lab showed that several different classes of DNA-binding motifs, from HTH to zinc fingers, utilized this mode of recognition (47). Similar to the 5′-pyrimidine of the 5′-YpG-3′ in the Ndt80-DNA structure, the Thy2 nucleobases in the B. subtilis CcpA–(HPr-Ser46-P)–DNA complexes all show significant displacement from optimal stacking with the following Gua3 as well as the hallmark stacking/van der Waals contact with the side chain of Arg22 (Figure 5A). However, the Arg22-Thy2 stacking may not be as optimal (~4.1 Å) as other 5′-YpG-3′ contacts, perhaps explaining why nucleotides 2 and 13 are not completely conserved in cre sites. In fact, analysis of the sequences of a number of cre sites shows that a thymine or pyrimidine is not strictly conserved at this location and in fact, in several cases is even a purine (Figure 1A). Regardless, the Arg22-(5′-YpG-3′) interaction combined with the Asn29 Cβ contact to Thy2 likely explains why a thymine is strongly preferred at cre position 2 (Figure 1B).

Aside from the complete conservation of guanine–cytosine base pairs 2/14 and 8/9 and the preference for a thymine/adenine at position 2/13, the other positions of the 16-bp cre are not conserved in cre sites and have been shown not to be important for CcpA-mediated transcription regulation (Figure 1A) (4,35). The structures show that these nucleotides are not recognized specifically by any CcpA residue, providing an explanation for this finding. In fact, the contacts that CcpA makes to these nucleotides are confined to van der Waals interactions, which lack strict chemical and geometrical restraints. In mediating its DNA contacts, CcpA utilizes non-polar side chains or the aliphatic portions of polar residues (Figure 5C). The residues used in these varied contacts are Ile6, Ser16, Met17, Ala18, Ala57 and the aliphatic portions of Tyr7 and Asn29. It is also of interest to note that while CcpA makes several water-mediated DNA phosphate backbone contacts there do not appear to be any solvent bridged protein–nucleobase interactions to any of the cre site bases. Perhaps the van der Waals contacts act to replace these commonly found interactions.

The large number of van der Waals contacts observed in the CcpA–cre complexes underscores the abundance of non-polar residues in the CcpA DNA-binding domain, particularly in its recognition helix (helix 2). It also suggests one reason why most cre sites are relatively rich in AT base pairs as non-polar side chains can partake in favourable interactions with the major groove-protruding methyl groups of thymines. Regardless, the non-polar side chains found in the CcpA DNA-binding domains have the capability of contacting any of the four nucleobases. Comparison of the three structures shows that the number of overall side chain–base contacts are very similar; the CcpA–(HPr-Ser46-P)–syn, CcpA–(HPr-Ser46-P)–ackA2 and CcpA–(HPr-Ser46-P)–gntR-down have 13, 13 and 14 side chain–base interactions, respectively (Figure 5C). While the gntR-down bound structure has more overall protein–DNA contacts, some of these contacts may be slightly unfavourable as they involve interactions between polar groups and hydrophobic groups, such as the Ala18-Cβ to Ade4 N6 interaction in one-half site and Ala18-Cβ to Gua13 O6 contact in the other half site. This contrasts with the non-polar or van der Waals contacts made by the Ala18 Cβ to thymine methyl groups observed in the syn and ackA2 structures. Thus, the non-polar residues in the CcpA DNA-binding domain contribute to binding affinity whilst allowing promiscuity in nucleobase interactions. Of course, another factor contributing to binding strength but not specificity are the numerous side chain–phosphate backbone interactions. There are 24 such contacts in each complex.

Like CcpA a number of bacterial transcription regulators function as global effectors of transcription by binding cognate DNA sites in the promoters of the genes they regulate. For example, the cAMP receptor protein (CRP), also known as CAP, functions analogously to the Gram-positive CcpA as the master regulator of carbon catabolite control in Gram-negative bacteria. CRP is activated to bind to its cognate 22-bp DNA site by first binding cAMP (49). Interestingly, unlike Gram-negative bacteria, Gram-positive bacteria do not normally contain cAMP, except under conditions of oxygen limitation. Thus, different mechanisms for CCR are clearly at play in Gram-negative compared to Gram-positive bacteria. Unlike CcpA, CRP, which regulates more than 200 genes, appears to bind its DNA sites with higher stringency, as 14 out of the 22 bp are recognized specifically (49). However, it remains to be seen whether CRP also displays some level of promiscuity in DNA binding. It would seem likely that all global transcription regulators would benefit from displaying some degree of plasticity in their DNA-binding capabilities. Further studies combining structural and biochemical analyses will be needed to address this important issue.

In summary, our structures of CcpA–(HPr-Ser46-P) bound to three divergent cre sites reveal two key features that help to explain how CcpA can bind cre sites with different DNA sequences but with similar affinities. First, the structures demonstrate that CcpA binds DNA using two flexibly attached DNA-binding modules: the HTHLH module and the hinge helix. The flexible linkage of the two modules permits them to dock favourably onto diverse DNA conformations, with conserved contacts between Arg22 and Gua3 primarily stabilizing the three helix bundle module onto the major grooves of each half site and the Leu56-CpG contacts locking the hinge helices into the DNA minor groove (Figure 6). Outside these G–C nucleotides, the other bases of the >50 cre sites show little conservation. This diversity is accommodated by the presence of a number of non-polar residues in the DNA-binding modules, particularly the HTH that can make numerous contacts that impart binding affinity without enforcing rigid specificity. In this way, CcpA can bind multiple sequences in the B. subtilis genome and function as a global regulator of transcription.

Figure 6.
Key properties that allow CcpA to function as a global regulator. The DNA-binding properties of CcpA that are key for its global function include the utilization of two separable DNA-binding modules, the HTHLH motifs, which contacts the major groove, ...

ACCESSION NUMBERS

Coordinates and structure factor amplitudes for the CcpA–(HPr-Ser46-P)–syn, CcpA–(HPr-Ser46-P)–ackA2 and CcpA–(HPr-Ser46-P)–gntR-down structures have been deposited with the Protein Data Bank under the accession codes 3OQO, 3OQM and 3OQN, respectively.

FUNDING

Funding for open access charge: MD Anderson Trust Fellowship; Burroughs Wellcome Career Development Award; National Institutes of Health (GM074815 to M.A.S.); Welch Foundation (G-0040 to R.G.B.); BMBF, BaCell-SysMO and Deutsche Forschungsgemeinschaft (SFB 476 to W.H.); Fonds der Chemischen Industrie (to W.H.).

Conflict of interest statement. None declared.

SUPPLEMENTARY DATA

Supplementary Data are available at NAR Online.

Supplementary Data:

ACKNOWLEDGEMENTS

We thank the Advanced Light Source (ALS) and their support staff. The ALS is supported by the Director, Office of Science, Office of Basic Energy Sciences and Material Science Division of the US Department of Energy at the Lawrence Berkeley National Laboratory. We also thank Gerald Seidel for constructing pWH653.

REFERENCES

1. Bruckner R, Titgemeyer F. Carbon catabolite repression in bacteria: choice of the carbon source and autoregulatory limitation of sugar utilization. FEMS Microbiol. Lett. 2002;209:141–148. [PubMed]
2. Stülke J, Hillen W. Coupling physiology and gene regulation in bacteria: the phosphotransferase sugar uptake system delivers the signals. Naturwissenschaften. 1998;85:583–592. [PubMed]
3. Stülke J, Hillen W. Regulation of carbon catabolism in Bacillus species. Annu. Rev. Microbiol. 2000;54:849–880. [PubMed]
4. Fujita Y. Carbon catabolite control and the metabolic network in Bacillus subtilis. Biosci. Biotechnol. Biochem. 2009;73:245–259. [PubMed]
5. Deutscher J. The mechanisms of carbon catabolite repression in bacteria. Curr. Opin. Microbiol. 2008;11:87–93. [PubMed]
6. Görke B, Stülke J. Carbon catabolite repression in bacteria: many ways to make the most of nutrients. Nat. Rev. Microbiol. 2008;6:613–624. [PubMed]
7. Warner JB, Lolkema JS. CcpA-dependent carbon catabolite repression in bacteria. Microbiol. Mol. Biol. Rev. 2003;67:475–490. [PMC free article] [PubMed]
8. Weickert MJ, Adhya S. A family of bacterial regulators homologous to Gal and Lac repressors. J. Biol. Chem. 1992;267:15869–15874. [PubMed]
9. Schumacher MA, Choi KY, Zalkin H, Brennan RG. Crystal structure of LacI member, PurR, bound to DNA: minor groove binding by alpha helices. Science. 1994;266:763–770. [PubMed]
10. Schumacher MA, Choi KY, Lu F, Zalkin H, Brennan RG. Mechanism of corepressor-mediated specific DNA binding by the purine repressor. Cell. 1995;83:147–155. [PubMed]
11. Schumacher MA, Allen GS, Diel M, Seidel G, Hillen W, Brennan RG. Structural basis for allosteric control of the transcription regulator CcpA by the phosphoprotein HPr-Ser46-P. Cell. 2004;118:731–741. [PubMed]
12. Bell CE, Lewis M. A closer view of the conformation of the Lac repressor bound to operator. Nat. Struct. Biol. 2000;7:209–214. [PubMed]
13. Bell CE, Lewis M. Crystallographic analysis of Lac repressor bound to natural operator O1. J. Mol. Biol. 2001;312:921–926. [PubMed]
14. Lewis M, Chang G, Horton NC, Kercher MA, Pace HC, Schumacher MA, Brennan RG, Lu P. Crystal structure of the lactose operon repressor and its complexes with DNA and inducer. Science. 1996;271:1247–1254. [PubMed]
15. Deutscher J, Küster E, Bergstedt U, Charrier V, Hillen W. Protein kinase-dependent HPr/CcpA interaction links glycolytic activity to carbon catabolite repression in gram-positive bacteria. Mol. Microbiol. 1995;15:1049–1053. [PubMed]
16. Henkin TM. The role of the CcpA transcriptional regulator in carbon catabolite metabolism in Bacillus subtilis. FEMS Microbiol. Lett. 1996;135:9–15. [PubMed]
17. Aung-Hilbrich LM, Seidel G, Wagner A, Hillen W. Quantification of the influence of HPrSer46P on CcpA-cre interaction. J. Mol. Biol. 2002;319:77–85. [PubMed]
18. Jones BE, Dossonnet V, Küster E, Hillen W, Deutscher J, Klevit RE. Binding of the catabolite repressor protein CcpA to its DNA target is regulated by phosphorylation of its corepressor HPr. J. Biol. Chem. 1997;272:26530–26535. [PubMed]
19. Galinier A, Deutscher J, Martin-Verstraete I. Phosphorylation of either Crh or HPr mediates binding of CcpA to the Bacillus subtilis xyn cre and catabolite repression of the xyn operon. J. Mol. Biol. 1999;286:307–314. [PubMed]
20. Audette GF, Engelmann R, Hengstenberg W, Deutscher J, Hayakama K, Quail JW, Delbaere LT. The 1.9 Å resolution structure of phospho-serine 46 HPr from Enterococcus faecalis. J. Mol. Biol. 2000;303:545–553. [PubMed]
21. Moreno MS, Schneider BL, Maile RR, Weyler W, Saier MH., Jr Catabolite repression mediated by the CcpA protein in Bacillus subtilis: novel modes of regulation revealed by whole-genome analyses. Mol. Microbiol. 2001;39:1366–1381. [PubMed]
22. Turinsky AJ, Grundy FJ, Kim JH, Chambliss GH, Henkin TM. Transcriptional activation of the Bacillus subtilis ackA gene requires sequences upstream of the promoter. J. Bacteriol. 1998;180:5961–5967. [PMC free article] [PubMed]
23. Moir-Blais TR, Grundy FJ, Henkin TM. Transcriptional activation of the Bacillus subtilis ackA promoter requires sequences upstream of the CcpA binding site. J. Bacteriol. 2001;183:2389–2393. [PMC free article] [PubMed]
24. Pesecan-Siedel E, Galinier Z, Longin R, Deutscher J, Danchin A, Glaser P, Martin-Verstraete I. Catabolite regulation of the pta gene as part of carbon flow pathways in Bacillus subtilis. J. Bacteriol. 1999;181:6889–6897. [PMC free article] [PubMed]
25. Shin BS, Choi SK, Park SH. Regulation of the Bacillus subtilis phosphotransacetylase gene. J. Biochem. 1999;126:333–339. [PubMed]
26. Nicholson WL, Park YK, Henkin TM, Won M, Weickert MJ, Gaskell JA, Chambliss GH. Catabolite repression-resistant mutations of the Bacillus subtilis alpha-amylase promoter affect transcription levels and are in an operator-like sequence. J. Mol. Biol. 1987;198:609–618. [PubMed]
27. Krüger S, Gerz S, Hecker M. Transcriptional analysis of bglPH expression in Bacillus subtilis: evidence for two distinct pathways mediating carbon catabolite repression. J. Bacteriol. 1996;177:5590–5597. [PMC free article] [PubMed]
28. Monedero V, Boel G, Deutscher J. Catabolite regulation of the cytochrome c550-encoding Bacillus subtilis cccA gene. J. Mol. Microbiol. Biotechnol. 2001;3:433–438. [PubMed]
29. Asai K, Baik SH, Kasahara Y, Moriya S, Ogasawara N. Regulation of the transport system for C4-dicarboxylic acids in Bacillus subtilis. Microbiology. 2000;146:263–271. [PubMed]
30. Darbon E, Servant P, Poncet S, Deutscher J. Antitermination by GlpP, catabolite repression via CCpA and inducer exclusion triggered by P-GlpK dephosphorylation control Bacillus subtilis glpFK expression. Mol. Microbiol. 2002;43:1039–1052. [PubMed]
31. Grundy FJ, Waters DA, Allen SHG, Henkin TM. Regulation of the Bacillus subtilis Acetate kinase gene by CcpA. J. Bacteriol. 1993;175:7348–7355. [PMC free article] [PubMed]
32. Puri-Taneja A, Paul S, Chen Y, Hulett FM. CcpA causes repression of phoPR promoter through a novel transcription start site. J. Bacteriol. 2006;188:1266–1278. [PMC free article] [PubMed]
33. Kim JH, Yang YK, Chambliss GH. Evidence that Bacillus catabolite control protein CcpA interacts with RNA polymerase to inhibit transcription. Mol. Microbiol. 2005;56:155–162. [PubMed]
34. Martin-Verstraete I, Stulke J, Klier A, Rapoport G. Two different mechanisms mediate catabolite repression of the Bacillus subtilis levanase operon. J. Bacteriol. 1995;177:6919–6927. [PMC free article] [PubMed]
35. Weickert MJ, Chambliss GH. Site-directed mutagenesis of a catabolite repression operator sequence in Bacillus subtilis. Proc. Natl Acad. Sci. USA. 1989;87:6238–6242. [PMC free article] [PubMed]
36. Miwa Y, Nakata A, Ogiwara A, Yamamoto M, Fujita Y. Evaluation and characterization of catabolite-responsive elements (cre) of Bacillus subtilis. Nucleic Acids Res. 2000;28:1206–1210. [PMC free article] [PubMed]
37. Seidel G, Diel M, Fuchsbauer N, Willen W. Quantitative interdependence of coeffectors, CcpA and cre in carbon catabolite regulation of Bacillus subtilis. FEBS J. 2005;272:2566–2577. [PubMed]
38. Lundblad JR, Laurance M, Goodman RH. Fluorescence polarization analysis of protein-DNA and protein-protein interactions. Mol. Endocrinol. 1996;10:607–612. [PubMed]
39. Horstmann N, Seidel G, Aung-Hilbrich LM, Hillen W. Residues His-15 and Arg-17 of HPr participate differently in catabolite signal processing via CcpA. J. Biol. Chem. 2007;282:1175–1182. [PubMed]
40. Chaptal V, Guegen-Chaignon V, Poncet S, Lecampion C, Meyer P, Deutscher J, Galingier A, Nessler S, Morera S. Structural analysis of B. subtilis CcpA effector binding site. Proteins. 2006;64:814–816. [PubMed]
41. Brünger AT, Adams PD, Clore GM, DeLano WL, Gros P, Crosse-Kunstleve RW, Jiang JS, Kuszewski J, Nilges M, Pannu NS, et al. Crystallography and NMR System: A new software suite for macromolecular structure determination. Acta Crystallogr. D Biol. Crystallogr. 1998;54:905–921. [PubMed]
42. Jones TA, Zou J-Y, Cowan SW, Kjeldgaard M. Improved methods for building protein models in electron density maps and the location of errors in these models. Acta. Crystallogr. 1991;A47:110–119. [PubMed]
43. Miwa Y, Nagura K, Eguchi S, Fukuda H, Deutscher J, Fujita Y. Catabolite repression of the Bacillus subtilis gnt operon exerted by two catabolite-responsive elements. Mol. Microbiol. 1997;23:1203–1213. [PubMed]
44. Lavery R, Moaker M, Maddocks JH, Petkeviciute D, Zakrzewska K. Conformational analysis of nucleic acids revisited: Curves+ Nucleic Acids Res. 2009;37:5917–5929. [PMC free article] [PubMed]
45. Peters JP, 3rd, Maher LJ. DNA curvature and flexibility in vitro and in vivo. Rev. Biophys. 2010;43:23–63. [PMC free article] [PubMed]
46. Lamoureux JS, Stuart D, Tsang R, Wu C, Glover JNM. Structure of the sporulation-specific transcription factor Ndt80 bound to DNA. EMBO J. 2002;21:5721–5732. [PMC free article] [PubMed]
47. Lamoureux JS, Maynes JT, Glover JNM. Recognition of 5′-YpG-3′ sequences by coupled stacking/hydrogen bonding interactions with amino acid residues. J. Mol. Biol. 2004;335:399–408. [PubMed]
48. Olson WK, Gorin AA, Lu XJ, Hock LM, Zhurkin VB. DNA sequence-dependent deformability deduced from protein-DNA crystal complexes. Proc. Natl Acad. Sci. USA. 1998;95:11163–11168. [PMC free article] [PubMed]
49. Lawson CL, Swigon D, Murakami KS, Darst SA, Berman HM, Ebright RH. Catabolite activator protein (CAP): DNA binding and transcription activation. Curr. Opin. Struct. Biol. 2004;14:10–20. [PMC free article] [PubMed]
50. Yoshida K, Aoyama D, Ishio I, Shibayama T, Fujita Y. Organization and transcription of the myo-inositol operon, io1, of Bacillus subtilis. J. Bacteriol. 1997;179:4591–4598. [PMC free article] [PubMed]
51. Miwa Y, Fujita Y. Involvement of two distinct catabolite-responsive elements in catabolite repression of the Bacillus subtilis myo-inositol (io1) operon. J. Bacteriol. 2001;183:5877–5884. [PMC free article] [PubMed]
52. Yoshida K, Ishio I, Nagakawa E, Yamamoto Y, Yamamoto M, Fujita Y. Systematic study of gene expression and transcription organization in the gntZ-ywaA region of Bacillus subtilis genome. Microbiology. 2000;146:573–579. [PubMed]
53. Choi SK, Saier MH., Jr Regulation of sigL expression by the catabolite control protein CcpA involves a roadblock mechanism in Bacillus subtilis: potential connection between carbon and nitrogen metabolism. J. Bacteriol. 2005;187:6856–6861. [PMC free article] [PubMed]
54. Yamamoto H, Murata M, Sekiguchi J. The CitST two-component system regulates the expression of the Mg-citrate transporter in Bacillus subtilis. Mol. Microbiol. 2000;37:898–912. [PubMed]
55. Delano WL. The PyMOL Molecular Graphics System. San Carlos, California: DeLano Scientific; 2002.
56. Parche S, Schmid R, Titgemeyer F. The phosphotransferase system (PTS) of Streptomyces coelicolor identification and biochemical analysis of a histidine phosphocarrier protein HPr encoded by the gene ptsH. Eur. J. Biochem. 1999;265:308–317. [PubMed]
57. Reizer J, Hoischen C, Titgemeyer F, Rivolta C, Rabus R, Stülke J, Karamata D, Saier MH, Jr, Hillen W. A novel protein kinase that controls carbon catabolite repression in bacteria. Mol. Microbiol. 1998;27:1157–1169. [PubMed]

Articles from Nucleic Acids Research are provided here courtesy of Oxford University Press
PubReader format: click here to try

Formats:

Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...

Links

  • MedGen
    MedGen
    Related information in MedGen
  • Nucleotide
    Nucleotide
    Published Nucleotide sequences
  • Protein
    Protein
    Published protein sequences
  • PubMed
    PubMed
    PubMed citations for these articles
  • Structure
    Structure
    Published 3D structures

Recent Activity

Your browsing activity is empty.

Activity recording is turned off.

Turn recording back on

See more...