- Research article
- Open Access
Crystal structures of an Extracytoplasmic Solute Receptor from a TRAP transporter in its open and closed forms reveal a helix-swapped dimer requiring a cation for α-keto acid binding
© Gonin et al; licensee BioMed Central Ltd. 2007
- Received: 19 October 2006
- Accepted: 15 March 2007
- Published: 15 March 2007
The import of solutes into the bacterial cytoplasm involves several types of membrane transporters, which may be driven by ATP hydrolysis (ABC transporters) or by an ion or H+ electrochemical membrane potential, as in the tripartite ATP-independent periplasmic system (TRAP). In both the ABC and TRAP systems, a specific periplasmic protein from the ESR family (Extracytoplasmic Solute Receptors) is often involved for the recruitment of the solute and its presentation to the membrane complex. In Rhodobacter sphaeroides, TakP (previously named SmoM) is an ESR from a TRAP transporter and binds α-keto acids in vitro.
We describe the high-resolution crystal structures of TakP in its unliganded form and as a complex with sodium-pyruvate. The results show a limited "Venus flytrap" conformational change induced by substrate binding. In the liganded structure, a cation (most probably a sodium ion) is present and plays a key role in the association of the pyruvate to the protein. The structure of the binding pocket gives a rationale for the relative affinities of various ligands that were tested from a fluorescence assay. The protein appears to be dimeric in solution and in the crystals, with a helix-swapping structure largely participating in the dimer formation. A 30 Å-long water channel buried at the dimer interface connects the two ligand binding cavities of the dimer.
The concerted recruitment by TakP of the substrate group with a cation could represent a first step in the coupled transport of both partners, providing the driving force for solute import. Furthermore, the unexpected dimeric structure of TakP suggests a molecular mechanism of solute uptake by the dimeric ESR via a channel that connects the binding sites of the two monomers.
- Rhodobacter Sphaeroides
- Nucleotide Binding Domain
- Dimeric Nature
Transport systems are required in all organisms to facilitate movement of nutrients and other solutes across biological membranes. In prokaryotes, several classes of transport systems have been defined on the basis of their subunit composition and mode of energization . The well-characterized ATP-binding cassette superfamily (ABC) represents one of the largest families of solute-specific transporters. In the ABC system, the driving force for solute transport across the membrane subunits is derived from ATP hydrolysis. In bacteria, solute uptake often requires the presentation of substrate by a high affinity Extracytoplasmic Solute Receptor (ESR, also called S- or P-BP for Solute or Periplasmic Binding Protein). The three dimensional structures of numerous ESRs specific for a wide range of substrates have been determined and, despite lack of sequence similarity, all were found to adopt a similar ternary fold [2, 3] where the substrate binding site is located at the interface of two α/β domains connected by a hinge. The transport cycle begins with substrate binding to the ESR, inducing a conformational change to a "closed form" whereby the solvent is excluded from the substrate (hence the model denomination as a "Venus flytrap"). The docking of the loaded ESR to the ABC complex triggers a conformational change of the latter, which induces the binding of ATP and its hydrolysis by the Nucleotide Binding Domain (NBD) . The ESRs thus play a key role in both the recruitment of the specific substrate and the control of ATP hydrolysis by the NBD.
The requirement for solute recognition by a periplasmic subunit prior to its translocation is not specific to ABCs since ESRs are also found in ATP-independent secondary transporters, the so-called Tripartite ATP-independent Periplasmic transporters (TRAP). In TRAP systems, the periplasmic ESR (often called the P subunit) is associated with two membrane components: a large transmembrane subunit involved in the translocation process (the M subunit) and a smaller membrane component of unknown function (the Q subunit). TRAP transporters lack the sequence signature characteristic of NBD, and biochemical evidences suggests that their driving force does not come from ATP but rather from the free energy stored in an electrochemical ion gradient across the cytoplasmic membrane . The molecular mechanisms encompassing e.g. the recognition of the solute-ESR complex and the coupling of the transport to the ion gradient remain unknown.
The TRAP family is widespread in prokaryotes, as predicted from sequence analysis of bacterial genomes . However, the physiological role of few of them has been elucidated since ligands for ESRs of TRAP transporters have only been evidenced for C4-dicarboxylate , ectoine , glutamate , xylulose , and sialic acid . The best characterized TRAP transporters at functional and molecular levels are the high-affinity C4-dicarboxylate transport system (dctPQM) from Rhodobacter capsulatus [5, 12] and the sialic acid transporter (SiaPQM) from Haemophilus influenzae . In the latter, the structure of the periplasmic subunit (SiaP) was solved very recently at high resolution, revealing, among others, an overall topology similar to ABC ESR proteins .
In this study, we have focussed on the structural characterization of SmoM, a member of the DctP family. The smoM gene was initially annotated as coding for a sorbitol/mannitol binding protein on the basis of its position in the genome, close to the smo operon encoding known sorbitol/mannitol catabolic genes . There is now clear evidence that SmoM does not participate in sorbitol or mannitol transport. First, the gene smoM is more than 500 bp away from the smo operon. Second, two genes homologous to dctQ and dctM are located in the region immediately downstream of SmoM, forming a putative functional TRAP transporter. Finally, purified proteins from the SmoM family neither bind sorbitol nor mannitol but display a specificity for α-keto acid complexes ( and this study), consistent with the suggested role of this transporter for supplying intermediates in the synthesis of valine and isoleucine. We thus propose to rename SmoM as TakP (TRAP transporter a lpha-k eto acid binding P subunit) and, by the same token, the associated membrane proteins as TakQ and TakM (the small and large integral membrane proteins, respectively).
In this paper, we present the high resolution structures of TakP in its unliganded form and complexed with sodium-pyruvate. This study reveals a key role for an ion in the attachment mode of the substrate, as well as an unexpected dimerization largely mediated by a helix swapping. The molecular mechanism of solute uptake is discussed in the light of these unique structural findings.
TakP, a secondary transporter of α-keto acids
We became initially interested in the study of TakP when we found that a Rhodobacter sphaeroides mutant carrying a single Tn5 insertion in takP displayed a higher resistance to selenite . Recently, TakP from R. capsulatus was shown to bind monocarboxylic 2-oxoacid anions in vitro . We carried out a phenotypic analysis of the takP mutant to determine the most physiologically relevant substrate of the Tak transporter. However, no phenotypic difference could be characterized when comparing mutant and parent strains cultivated in minimal media supplemented with various α-keto acids (not shown). This suggests the presence of another import system in vivo or a non essential role for this ESR in the transport process.
We overexpressed and purified TakP from Rhodobacter sphaeroides and confirmed its ability to bind a range of α-keto acids. A general feature of ESRs is that substrate binding is accompanied by a diminished fluorescence from some tryptophan residue(s) as a result of the conformational changes induced by the binding. Indeed, we found that about 30% of the tryptophan fluorescence emitted by TakP became quenched when adding a saturating concentration of substrate. This was accompanied by a shift of the emission peak: the difference spectrum between the unliganded and liganded (quenched) protein has its maximum around 345 nm, whereas the bulk fluorescence from the unliganded form peaks at 335 nm. These features suggest that the tryptophans which become quenched in the liganded configuration represent a more solvent-exposed fraction of the protein tryptophans in the unliganded structure. There are 10 Trp residues in the TakP sequence. From the structural information describe below, it turned out that one of these Trp residues (Trp 215) is directly interacting with the ligand when present, so that its fluorescence may be strongly quenched as a result. Two others undergo a significant displacement during the open/closed transition, which may also affect their fluorescence properties. Clearly, the observed amplitude of the fluorescence quenching caused by ligand binding (~30%) implies that these sensitive residues have for some reason a larger relative contribution to the fluorescence emission than the other tryptophans of the protein.
Here, F is the fluorescence amplitude and F0 its value in the absence of ligand. Δ F is the normalized amplitude of the saturated quenching, [PL] is the concentration of liganded protein, [P0] and [L0] are the concentrations of the total protein and ligand, respectively. The protein concentration was determined from its 280 nm absorbance and pertains here to the monomeric unit (see below). Figure 1A shows the change of fluorescence amplitude as a function of added pyruvate. The solid line shows the best fit obtained using the above equation, yielding K d ≈ 0.26 μM.
As described below, it appeared that the protein was in fact homodimeric and one may wonder whether any cooperativity is taking place between the two monomers. In fact, the satisfactory fit with a simple binding function excludes that significant cooperativity or anticooperativity be present. This is illustrated by the dashed line that was computed by simulating a small cooperativity (see legend) and clearly represents the upper limit that could accommodate the data in this respect. The titration experiments show that the binding occurs on a single, homogeneous site. To ascertain that this site corresponds to the monomeric unit (rather than, e.g., to the dimer), we also ran (data not shown) experiments at high protein concentrations (> Kd). Under such conditions, the binding titration (or its initial part if [P0] is not very large with respect to Kd) is essentially linear (all the added substrate is bound until saturation) and the concentration of binding sites is easily determined from the slope. The results confirmed that the number of binding sites was ~1 per monomer and that the protein was ~100% active for binding the substrate – in agreement with the crystal structure described in the following.
The K d values were determined for different structurally-related compounds as shown in Figure 1B, C and 1D. No binding was observed with α-ketoglutarate. In all cases the trend is the same as observed by Thomas et al . The length of the aliphatic backbone chain clearly influences the affinity, a result that will be discussed later in the light of the structure. We next focus on the structural characterization of the interactions of TakP with 2-oxoacids, using pyruvate as a model substrate.
A dimeric venus-flytrap with a swapped helix
Summary of crystal parameters, data collection and refinement statistics
Unbound Selenomethionine (P 21)
Pyruvate (C 2)
Wavelength, Å a
Resolution range, Å
No. of measured reflections
No. of unique reflections
R sym b,c
Completeness, % b
Resolution range, Å
No. of non hydrogen atoms:
Average B-factors, Å 2 :
RMSD bonds, Å
RMSD angles, °
Additional file 2: A movie depicting the transition between the open – closed transition in TakP. The coloring scheme in this movie is according to the domains as they are defined in Figure 3. It is apparent that the movement of domain 2 on one monomer is somehow hindered by the swapped helix of the other monomer. (MOV 2 MB)
A conspicuous feature of the dimeric association in TakP is the presence of a water-filled channel buried at the dimer interface, which spans 30 Å from one ligand binding cavity to the other. As discussed later, we believe that substrate translocation through this connecting cavity may play a functional role.
Co-recognition of a cation with pyruvate
In the complex structure, the acidic moiety of the pyruvate is involved in a salt bridge with Arg177 and one oxygen atom is H-bonded to Tyr100. The central feature for the binding of the pyruvate to the protein is the presence of a cation (Figure 6A). This cation has a bi-pyramidal coordination with a square base. The four equatorial positions are provided by the O3 of pyruvate, the main chain carbonyl oxygen of Trp215 and a bi-dentate and mono-dentate ligand provided by the side chains of Glu214 and Glu240, respectively. The apical positions are occupied on one side by an oxygen atom from the acidic moiety of pyruvate and, on the other side, by the Oδ1 of the side chain of Gln156. The measured distances between the cation and the six oxygen atoms range from 2.34 Å to 2.43 Å. These values are very close to the canonical distances expected for a magnesium or a sodium ion (RLi = 2.14 Å; RMg = RNa = 2.46 Å ; RCa = 2.66 Å ; RK = 2.77 Å [23, 24]). Since only sodium salts were present in our crystallization conditions this cation can be safely identified as a sodium ion. Among the six residues involved in the recognition of sodium-pyruvate, only one (Tyr100) is provided by domain I, while the others belong to domain II or to the hinge (Figure 6A).
Structural changes upon sodium pyruvate binding
Two kinds of conformational changes occur upon complex formation. First, there is a 14° rigid body rotation of domain II (Figure 6B; rotation was calculated using the DYNDOM program). Indeed, superimposition of the liganded and unliganded structures results in a r.m.s. deviation of 1.6Å for 334 Cα positions, a value that is an average of a high r.m.s. deviation measured for domain II (3.3Å for 89 Cα positions) and a rather low value for the rest of the molecule, comprising domain I, the clamp and the swapped helix (0.6Å for 245 Cα positions). The inter-domain closing is dominated by van der Waals contacts with only one hydrogen bond (Tyr99OH – Glu240Oε2) between domains I and II in the closed form. The dimerization interface is not modified by the open/closed transition, i.e. the intermolecular hydrogen bonds and salt bridges are conserved. Only one salt bridge (Glu340A-Lys289B) is specific to the closed conformation. Because of the absence of the symmetric salt bridge (Lys289A-Glu340B), the dimer appears slightly asymmetric.
The second conformational change associated with ligand binding corresponds to a small but significant structural rearrangement inside domain II, reflected by a r.m.s. deviation of 1.2 Å after superimposition of the 89 Cα positions of this domain in both structures. This rearrangement is mainly located in a loop-helix-loop region comprising residues 178 to 201, a portion of the structure that is not involved in the direct binding of sodium or of pyruvate. The movement of this region upon substrate binding locks the inter-domain closing by increasing the fit between both domains, which results in a ligand binding cavity completely shielded from the external solvent (Figure 6C and 6D). On the other hand, the internal water channel connecting the binding cavities is not affected by the open/closed transition.
Ligand binding kinetics determined for numerous ESRs from ABC transporters by stopped-flow fluorescence spectroscopy have revealed a single-step equilibrium binding process. These data suggest that the protein is stable in the open unliganded conformation, and that ligand binding triggers the closing of the globular domains. This model has been supported by crystallographic studies, which provided evidence for the existence of three different conformational states of ESRs: an open unliganded form, an open liganded form and a closed liganded form . In the case of ESRs from the DtcP family, an uncommon kinetic behavior was reported , since the rate of substrate binding decreased when increasing its concentration. A model was proposed, involving a fourth ("closed unliganded") form of the protein. The binding would occur through the equilibrium between this predominant, non-binding, form and the open, binding configuration . Our data show that the unliganded TakP was crystallized in the open configuration. This does not exclude the possibility that a more stable closed form might exist in solution, but it makes this hypothesis less likely.
Despite the very low sequence identity, TakP has been previously classified into family 7 of ESRs in the Pfam database. The high resolution crystal structure of TakP confirms an ESR overall fold. However, two additional secondary structure elements, a "clamp" and a helix swap, were not anticipated from primary sequence analysis. The topology and location of the clamp suggests a structural role in restricting the rigid body movement of domain II upon substrate binding. The restricted opening of TakP caused by the clamp appears when comparing the liganded and unliganded structures of ESRs. The two β-strands hinge allows a rather large rotation of domain II upon ligand binding (from 17° for the Nickel- to 56° for D-ribose- binding proteins; the average is 45°) whereas it is significantly smaller in TakP (14°) and below the average in SiaP (27°). The swapped helix also largely contributes to the limited opening of TakP as can be viewed in a movie provided as additional file 2. The requirement for a restricted movement upon solute binding might be important for the energetics of ligand binding. Since the residues responsible for the binding of the substrate belong almost exclusively to domain II, the proximity of the two domains in the apo state may facilitate the substrate-induced closing.
As revealed by the present work, a sodium ion plays a key role for the binding of the 2-oxo acids to the protein. Since TRAP transporters utilize the transmembrane electrochemical Na+ or H+ gradient as the driving force for solute import, it is tempting to believe that the concerted recruitment by the ESR of the substrate group with a cation is a first step in the coupled transport of both partners .
The presence of a swapped helix in TakP was an original and unanticipated feature. The 40 swapped residues significantly contribute to the total surface that is buried in the dimer, therefore playing a clear role in the dimer formation. About a hundred proteins were found to be homologue to TakP and they all have in common the long C-terminal extension corresponding to the swapped helix. Because of its importance in dimerization this helix may be a marker of a novel family of dimeric ESRs. This dimeric nature of TakP is intriguing because ESRs, especially when associated with an ABC transporter, are believed to be monomeric. To our knowledge, there is one report of dimer formation, based on biochemical evidence . However, sequencing has now revealed the presence of ABC transmembrane dimeric subunits directly fused to one or two ESRs, which implies that two or four binding sites are present per functional translocation unit . Multimerization of ESRs that are not associated to ABC transport systems is exceptional and then appears linked to a particular function: activation of transport in glutamate receptors (a close structural homolog of TakP found by DALI) and activation/repression of DNA translation by DNA-repressor of the LacR family. In lactoferrin and transferrin, two ESRs are fused into a single protein and are therefore associated as a "forced dimer" . The role associated with the dimerization of TakP remains to be investigated. Our binding data exclude any significant cooperativity between the two sites, which is consistent with the structural results showing no significant modification of the monomer/monomer interfacial regions upon binding the ligand. A possible role for the dimerization of TakP is proposed below.
The X-ray structures of TakP solved in the presence and in the absence of substrate reveal the structural determinants responsible for the binding of α-keto acids. The requirement of a cation for the binding of the ligand is suggestive of a role in the energization of the transport. Moreover, an unexpected helix-swapped dimer is observed in two different crystal forms. Although this quaternary structure does not generate a cooperative binding of the substrate, the connecting channel at the dimeric interface could be involved in the translocation process.
Vector pET101/D-TOPO (Invitrogen) containing a T7 promoter, a C-Terminal His6 tag, and V5 epitope was used for cloning and expression. Two synthetic oligonucleotide primers were designed in order to amplify the TakP gene from Rhodobacter sphaeroides 2.4.1 genomic DNA. The 1099 bp fragment obtained after amplification was electrophoretically separated on a 1% SeaKem GTG-agarose gel and extracted prior to cloning into pET101/D-TOPO.
Bacterial expression and protein purification
The recombinant protein was overexpressed in E. coli BL21 strain. Cells were allowed to grow in LB (Lenox Broth) medium containing 100 mg/ml ampicilline to an OD600 of 0.7 before inducing expression with 1 mM Isopropyl-β-D-thiogalactopyranoside (IPTG) followed by 20 hours incubation at 30°C. The cells were pelleted, resuspended in buffer A containing 50 mM phosphate pH 8.0, 450 mM NaCl, and disrupted with a French Press at 7 Mpa. The resulting soluble fraction was loaded on a Nickel charged column (HisTrap column, Amersham) and the protein was eluted by an imidazole step gradient (40 mM wash and 200 mM elution). The recombinant selenomethionine labeled protein was overexpressed in E. coli after growth in a 1 L of methionine-minus medium from Molecular Dimensions, complemented with 40 mg of L-selenomethionine (SeMet), L-lysine, L-threonine and L-phenylalanine as described . Purification of the SeMet TakP was performed as previously, except the addition of 1 mM Tris(2-carboxyethyl)phosphine (TCEP) in the different buffers.
Cross-linking and gel filtration chromatography
The cross-linking experiment was performed by incubating 3.2 and 6.3 μM TakP with 50 mM glutaraldehyde, in 20 mM Na2HPO4/KH2PO4 pH 7.8, at 18°C for 3 hours. The control reaction contained no cross-linker. The denaturing gel electrophoresis was done with a 10% Nu-PAGE gel (Invitrogen), in MOPS buffer. The gel filtration chromatography was done using a Superdex 200 26/60 column (Amersham Biosciences) equilibrated with 20 mM Tris HCl (pH 8.0), 50 mM NaCl. The column was previously size calibrated using commercial gel filtration standards (Amersham Biosciences).
For crystallization, the native protein was exchanged into buffer B (50 mM Tris HCl pH 8.5, 180 mM NaCl) and concentrated up to 15 mg.ml-1. All the crystallization experiments were carried out at 293 K using the hanging drop vapor diffusion technique. Crystals of the unliganded protein were obtained by mixing 2 μl of protein with 2 μl of a reservoir solution (500 μl) containing 100 mM sodium citrate (pH 5.8–6.0) and 1.4–1.6 M ammonium sulfate. In these conditions, three different crystal morphologies were obtained: cylindrical rods, large hexagonal crystals and, more rarely, a large stacking of finely faceted plate crystals. Only crystals extracted from this bundles diffract x-rays. They grew in about five days and belong to space group P 21 (Table 1). In order to get a structure of a pyruvate complex we re-screened various co-crystallization conditions with 30 mM pyruvate. Crystals were obtained in approximately the same conditions as for the native, i.e. by mixing 2 μl of the native protein with 2 μl of a reservoir solution containing 100 mM sodium citrate (pH 5.4), 1.4 M ammonium sulfate and 30 mM sodium pyruvate. Crystals grew in about 1 week and correspond to a different crystal form (Table 1).
Data collection and phasing
Native and SeMet crystals were cooled to 100 K after soaking for several minutes in a cryobuffer containing 30% glycerol whereas paraffin oil was used as cryoprotectant for the pyruvate-TakP crystals. Diffraction data on both the Se-Met labeled protein and the protein pyruvate complex crystals were collected at beamline ID23 (ESRF, France). The data sets were processed with MOSFLM  and subsequent data reduction was carried out using the CCP4 suite .
Structures determination and refinement
The structure of SeMet TakP was solved by the MAD method using data collected at three wavelengths. Fourty selenium positions were found from the MAD data by the program SOLVE . The four operators relating the four molecules in the asymmetric unit were found by the program and approximately 75% of the molecule was subsequently automatically built. Several rounds of iterative model building and refinement were performed using the programs COOT  and REFMAC . The final model contains four molecules (from residue 28 or 32 to 365), 760 solvent molecules and four molecules of glycerol. The structure of the protein in the presence of pyruvate was subsequently solved by molecular replacement using the unliganded structure as a search domain. It quickly appeared that domain II had a different orientation than in the native structure. The prime and switch option of SOLVE was used to increase the quality of the electron density map and the resulting map was then easily interpretable. After several cycles of model building and refinement with REFMAC, the final model contained 2 molecules of TakP, 2 sodium pyruvate complexes and 470 solvent molecules. In both structures, the structural parameters were consistently better than or within the average for structures at comparable resolution .
Fluorescence spectroscopy was performed using a Varian Cary Eclipse spectrofluorimeter with an excitation wavelength of 290 nm. The emission spectra were recorded between 300 and 500 nm. Ligand binding was determined from the partial quenching of this fluorescence emission. To gain a more accurate determination of the dissociation constant, the protein concentration was lowered down to 50 nM (in 50 mM Tris/HCl, pH 7) and the amplitude of the fluorescence emission was computed from an integration of the emission over the 315 nm to 360 nm range.
We would like to thank the staff of the ID23 and BM30 beamlines (ESRF, Grenoble France), Bernard Fernandez (SBTN, CEA-Marcoule) for technical assistance, and the "Programme de Toxicologie Nucléaire Environnementale" of the Commissariat à l'Energie Atomique for financial support.
- Saier MH Jr., Tran CV, Barabote RD: TCDB: the Transporter Classification Database for membrane transport protein analyses and information. Nucleic Acids Res 2006, 34(Database issue):D181–6. 10.1093/nar/gkj001PubMed CentralView ArticlePubMedGoogle Scholar
- Fukami-Kobayashi K, Tateno Y, Nishikawa K: Domain dislocation: a change of core structure in periplasmic binding proteins in their evolutionary history. J Mol Biol 1999, 286(1):279–290. 10.1006/jmbi.1998.2454View ArticlePubMedGoogle Scholar
- Quiocho FA, Ledvina PS: Atomic structure and specificity of bacterial periplasmic receptors for active transport and chemotaxis: variation of common themes. Mol Microbiol 1996, 20(1):17–25. 10.1111/j.1365-2958.1996.tb02484.xView ArticlePubMedGoogle Scholar
- Higgins CF, Linton KJ: The ATP switch model for ABC transporters. Nat Struct Mol Biol 2004, 11(10):918–926. 10.1038/nsmb836View ArticlePubMedGoogle Scholar
- Forward JA, Behrendt MC, Wyborn NR, Cross R, Kelly DJ: TRAP transporters: a new family of periplasmic solute transport systems encoded by the dctPQM genes of Rhodobacter capsulatus and by homologs in diverse gram-negative bacteria. J Bacteriol 1997, 179(17):5482–5493.PubMed CentralPubMedGoogle Scholar
- Rabus R, Jack DL, Kelly DJ, Saier MH Jr.: TRAP transporters: an ancient family of extracytoplasmic solute-receptor-dependent secondary active transporters. Microbiology 1999, 145 ( Pt 12): 3431–3445.View ArticleGoogle Scholar
- Ullmann R, Gross R, Simon J, Unden G, Kroger A: Transport of C(4)-dicarboxylates in Wolinella succinogenes. J Bacteriol 2000, 182(20):5757–5764. 10.1128/JB.182.20.5757-5764.2000PubMed CentralView ArticlePubMedGoogle Scholar
- Grammann K, Volke A, Kunte HJ: New type of osmoregulated solute transporter identified in halophilic members of the bacteria domain: TRAP transporter TeaABC mediates uptake of ectoine and hydroxyectoine in Halomonas elongata DSM 2581(T). J Bacteriol 2002, 184(11):3078–3085. 10.1128/JB.184.11.3078-3085.2002PubMed CentralView ArticlePubMedGoogle Scholar
- Quintero MJ, Montesinos ML, Herrero A, Flores E: Identification of genes encoding amino acid permeases by inactivation of selected ORFs from the Synechocystis genomic sequence. Genome Res 2001, 11(12):2034–2040. 10.1101/gr.196301PubMed CentralView ArticlePubMedGoogle Scholar
- Plantinga TH, Van Der Does C, Badia J, Aguilar J, Konings WN, Driessen AJ: Functional characterization of the Escherichia coli K-12 yiaMNO transport protein genes. Mol Membr Biol 2004, 21(1):51–57. 10.1080/09687680310001607369View ArticlePubMedGoogle Scholar
- Severi E, Randle G, Kivlin P, Whitfield K, Young R, Moxon R, Kelly D, Hood D, Thomas GH: Sialic acid transport in Haemophilus influenzae is essential for lipopolysaccharide sialylation and serum resistance and is dependent on a novel tripartite ATP-independent periplasmic transporter. Mol Microbiol 2005, 58(4):1173–1185. 10.1111/j.1365-2958.2005.04901.xView ArticlePubMedGoogle Scholar
- Janausch IG, Zientz E, Tran QH, Kroger A, Unden G: C4-dicarboxylate carriers and sensors in bacteria. Biochim Biophys Acta 2002, 1553(1–2):39–56. 10.1016/S0005-2728(01)00233-XView ArticlePubMedGoogle Scholar
- Muller A, Severi E, Mulligan C, Watts AG, Kelly DJ, Wilson KS, Wilkinson AJ, Thomas GH: Conservation of structure and mechanism in primary and secondary transporters exemplified by SiaP, a sialic acid-binding virulence factor from Haemophilus influenzae. J Biol Chem 2006, 281(31):22212–22222. 10.1074/jbc.M603463200View ArticlePubMedGoogle Scholar
- Stein MA, Schafer A, Giffhorn F: Cloning, nucleotide sequence, and overexpression of smoS, a component of a novel operon encoding an ABC transporter and polyol dehydrogenases of Rhodobacter sphaeroides Si4. J Bacteriol 1997, 179(20):6335–6340.PubMed CentralPubMedGoogle Scholar
- Thomas GH, Southworth T, Leon-Kempis MR, Leech A, Kelly DJ: Novel ligands for the extracellular solute receptors of two bacterial TRAP transporters. Microbiology 2006, 152(Pt 1):187–198. 10.1099/mic.0.28334-0View ArticlePubMedGoogle Scholar
- Pierru B, Grosse S, Pignol D, Sabaty M: Genetic and biochemical evidence for the involvement of a molybdenum-dependent enzyme in one of the selenite reduction pathways of Rhodobacter sphaeroides f. sp. denitrificans IL106. Appl Environ Microbiol 2006, 72(5):3147–3153. 10.1128/AEM.72.5.3147-3153.2006PubMed CentralView ArticlePubMedGoogle Scholar
- Saha RP, Bahadur RP, Pal A, Mandal S, Chakrabarti P: ProFace: a server for the analysis of the physicochemical features of protein-protein interfaces. BMC Struct Biol 2006, 6: 11. 10.1186/1472-6807-6-11PubMed CentralView ArticlePubMedGoogle Scholar
- Holm L, Sander C: Protein structure comparison by alignment of distance matrices. J Mol Biol 1993, 233(1):123–138. 10.1006/jmbi.1993.1489View ArticlePubMedGoogle Scholar
- Schiefner A, Breed J, Bosser L, Kneip S, Gade J, Holtmann G, Diederichs K, Welte W, Bremer E: Cation-pi interactions as determinants for binding of the compatible solutes glycine betaine and proline betaine by the periplasmic ligand-binding protein ProX from Escherichia coli. J Biol Chem 2004, 279(7):5588–5596. 10.1074/jbc.M309771200View ArticlePubMedGoogle Scholar
- Jin R, Gouaux E: Probing the function, conformational plasticity, and dimer-dimer contacts of the GluR2 ligand-binding core: studies of 5-substituted willardiines and GluR2 S1S2 in the crystal. Biochemistry 2003, 42(18):5201–5213. 10.1021/bi020632tView ArticlePubMedGoogle Scholar
- Cho Y, Sharma V, Sacchettini JC: Crystal structure of ATP phosphoribosyltransferase from Micobacterium tuberculosis. J Biol Chem 2003, 278(10):8333–8339. 10.1074/jbc.M212124200View ArticlePubMedGoogle Scholar
- Elcock AH, McCammon JA: Identification of protein oligomerization states by analysis of interface conservation. Proc Natl Acad Sci U S A 2001, 98(6):2990–2994. 10.1073/pnas.061411798PubMed CentralView ArticlePubMedGoogle Scholar
- Brown ID, Wu KK: Empirical parameters for calculating cation-oxygen bond valences. Acta Crystallogr B 1976, B32: 1957–1959. 10.1107/S0567740876006869View ArticleGoogle Scholar
- Nayal M, Di Cera E: Valence screening of water in protein crystals reveals potential Na+ binding sites. J Mol Biol 1996, 256(2):228–234. 10.1006/jmbi.1996.0081View ArticlePubMedGoogle Scholar
- Walmsley AR, Shaw JG, Kelly DJ: The mechanism of ligand binding to the periplasmic C4-dicarboxylate binding protein (DctP) from Rhodobacter capsulatus. J Biol Chem 1992, 267(12):8064–8072.PubMedGoogle Scholar
- Jacobs MH, van der Heide T, Driessen AJ, Konings WN: Glutamate transport in Rhodobacter sphaeroides is mediated by a novel binding protein-dependent secondary transport system. Proc Natl Acad Sci U S A 1996, 93(23):12786–12790. 10.1073/pnas.93.23.12786PubMed CentralView ArticlePubMedGoogle Scholar
- Richarme G: Associative properties of the Escherichia coli galactose-binding protein and maltose-binding protein. Biochim Biophys Acta 1983, 748(1):99–108.View ArticlePubMedGoogle Scholar
- van der Heide T, Poolman B: ABC transporters: one, two or four extracytoplasmic substrate-binding sites? EMBO Rep 2002, 3(10):938–943. 10.1093/embo-reports/kvf201PubMed CentralView ArticlePubMedGoogle Scholar
- Anderson BF, Baker HM, Dodson EJ, Norris GE, Rumball SV, Waters JM, Baker EN: Structure of human lactoferrin at 3.2-A resolution. Proc Natl Acad Sci U S A 1987, 84(7):1769–1773. 10.1073/pnas.84.7.1769PubMed CentralView ArticlePubMedGoogle Scholar
- Davidson AL, Chen J: ATP-binding cassette transporters in bacteria. Annu Rev Biochem 2004, 73: 241–268. 10.1146/annurev.biochem.73.011303.073626View ArticlePubMedGoogle Scholar
- Ames GF, Liu CE, Joshi AK, Nikaido K: Liganded and unliganded receptors interact with equal affinity with the membrane complex of periplasmic permeases, a subfamily of traffic ATPases. J Biol Chem 1996, 271(24):14264–14270. 10.1074/jbc.271.24.14264View ArticlePubMedGoogle Scholar
- Chen J, Sharma S, Quiocho FA, Davidson AL: Trapping the transition state of an ATP-binding cassette transporter: evidence for a concerted mechanism of maltose transport. Proc Natl Acad Sci U S A 2001, 98(4):1525–1530. 10.1073/pnas.041542498PubMed CentralView ArticlePubMedGoogle Scholar
- Davidson AL: Mechanism of coupling of transport to hydrolysis in bacterial ATP-binding cassette transporters. J Bacteriol 2002, 184(5):1225–1233.PubMed CentralView ArticlePubMedGoogle Scholar
- van der Heide T, Stuart MC, Poolman B: On the osmotic signal and osmosensing mechanism of an ABC transport system for glycine betaine. Embo J 2001, 20(24):7022–7032. 10.1093/emboj/20.24.7022PubMed CentralView ArticlePubMedGoogle Scholar
- Vivares D, Arnoux P, Pignol D: A papain-like enzyme at work: native and acyl-enzyme intermediate structures in phytochelatin synthesis. Proc Natl Acad Sci U S A 2005, 102(52):18848–18853. 10.1073/pnas.0505833102PubMed CentralView ArticlePubMedGoogle Scholar
- Leslie AGW: Autoindexing of rotation diffracton images and parameter refinement: 29–30 January 1993; SERC Daresbury Laboratory, Daresbury,UK. Edited by: Sawyer L, Isaacs N, Bailey S. ; 1993:44–51.Google Scholar
- CCP4: The CCP4 suite: programs for protein crystallography. Acta Crystallogr D Biol Crystallogr 1994, 50: 760–63.Google Scholar
- Terwilliger TC: SOLVE and RESOLVE: automated structure solution and density modification. Methods Enzymol 2003, 374: 22–37.View ArticlePubMedGoogle Scholar
- Emsley P, Cowtan K: Coot: model-building tools for molecular graphics. Acta Crystallogr D Biol Crystallogr 2004, 60(Pt 12 Pt 1):2126–2132. 10.1107/S0907444904019158View ArticlePubMedGoogle Scholar
- Murshudov GN, Vagin AA, Dodson EJ: Refinement of macromolecular structures by the maximum-likelihood method. Acta Crystallogr D Biol Crystallogr 1997, 53(Pt 3):240–255. 10.1107/S0907444996012255View ArticlePubMedGoogle Scholar
- Laskowski RA, MacArthur MW, Moss DS, Thornton JM: PROCHECK: a program to check the stereochemical quality of protein structures. J Appl Crystallogr 1993, 26: 283–291. 10.1107/S0021889892009944View ArticleGoogle Scholar
- Landau M, Mayrose I, Rosenberg Y, Glaser F, Martz E, Pupko T, Ben-Tal N: ConSurf 2005: the projection of evolutionary conservation scores of residues on protein structures. Nucleic Acids Res 2005, 33(Web Server issue):W299–302. 10.1093/nar/gki370PubMed CentralView ArticlePubMedGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.