PMCCPMCCPMCC

Search tips
Search criteria 

Advanced

 
Logo of actafjournal home pagethis articleInternational Union of Crystallographysearchsubscribearticle submission
 
Acta Crystallogr Sect F Struct Biol Cryst Commun. Jul 1, 2012; 68(Pt 7): 738–743.
Published online Jun 22, 2012. doi:  10.1107/S1744309112019124
PMCID: PMC3388911
Structure of Leishmania major cysteine synthase
Paul K. Fyfe,a Gareth D. Westrop,b Tania Ramos,c Sylke Müller,c Graham H. Coombs,c and William N. Huntera*
aDivision of Biological Chemistry and Drug Discovery, College of Life Sciences, University of Dundee, Dundee DD1 5EH, Scotland
bStrathclyde Institute of Pharmacy and Biomedical Sciences, University of Strathclyde, Glasgow G4 0RE, Scotland
cInstitute of Infection, Immunity and Inflammation, Wellcome Trust Centre for Molecular Parasitology, College of Medical, Veterinary and Life Sciences, University of Glasgow, Glasgow G12 8TA, Scotland
Correspondence e-mail: w.n.hunter/at/dundee.ac.uk
Received February 20, 2012; Accepted April 28, 2012.
Cysteine biosynthesis is a potential target for drug development against parasitic Leishmania species; these protozoa are responsible for a range of serious diseases. To improve understanding of this aspect of Leishmania biology, a crystallographic and biochemical study of L. major cysteine synthase has been undertaken, seeking to understand its structure, enzyme activity and modes of inhibition. Active enzyme was purified, assayed and crystallized in an orthorhombic form with a dimer in the asymmetric unit. Diffraction data extending to 1.8 Å resolution were measured and the structure was solved by molecular replacement. A fragment of γ-poly-d-glutamic acid, a constituent of the crystallization mixture, was bound in the enzyme active site. Although a d-­glutamate tetrapeptide had insignificant inhibitory activity, the enzyme was competitively inhibited (K i = 4 µM) by DYVI, a peptide based on the C-­terminus of the partner serine acetyltransferase with which the enzyme forms a complex. The structure surprisingly revealed that the cofactor pyridoxal phosphate had been lost during crystallization.
Keywords: Arabidopsis thaliana, cysteine synthase, Leishmania major
Leishmania, a widespread and important protozoan pathogen of humans and animals, requires cysteine for protein biosynthesis and as a precursor of trypanothione, a glutathione–spermidine conjugate unique to trypanosomatids with an essential role in redox metabolism and antioxidant defence (Krauth-Siegel & Comini, 2008 [triangle]). Cysteine is also the source of reduced sulfur for the biosynthesis of important metabolites such as coenzyme A, enzyme cofactors and iron–sulfur clusters (Nozaki et al., 2005 [triangle]). The vital role of cysteine raises the questions of how Leishmania obtains the amino acid, how cysteine metabolism in Leishmania might differ from that in the mammalian host and whether such differences might be targeted in drug-discovery research. L. major does not have a high-affinity transporter for the uptake of cysteine, but it can acquire methionine and, like the mammalian host, it has the enzymes required to convert methionine to cysteine by transsulfuration (Williams et al., 2009 [triangle]). The parasite can also produce cysteine from serine in a two-step process (Williams et al., 2009 [triangle]). Firstly, serine acetyltransferase (SAT) generates O-acetylserine (OAS) to supply the substrate for the second stage, which is catalyzed by the pyridoxal phosphate (PLP)-dependent cysteine synthase (CS; EC 2.5.1.47). This de novo pathway for cysteine biosynthesis is found in plants, bacteria and some protozoa, but is absent from mammals. In principle, L. major CS (LmCS) may represent a drug target, and an improved understanding of the enzyme might usefully inform on its potential in this respect. In particular, knowledge of the structure can support the development of reagents to chemically validate the target or to provide early-stage information on inhibitors (Hunter, 2009 [triangle]).
Some types of CS, including bacterial O-acetylserine sulfhydrylase type A (OASS-A) and plant O-acetylserine thiol-lyase (OAS-TL), combine reversibly with SAT to form a bi-enzyme complex in which SAT is active and CS is strongly inhibited (Campanini et al., 2005 [triangle]). The substrates of CS are effectors of complex formation; the complex is dissociated by elevated levels of OAS but is stabilized by sulfide. The complexes formed in plants and bacteria have distinctive features that indicate different regulatory functions (Salsi, Campanini et al., 2010 [triangle]; Wirtz et al., 2010 [triangle]). It has been established that the C-terminal end of SAT is critical for its interaction with CS and, in particular, all SATs possess a C-terminal isoleucine which is essential for CS binding. Peptides corresponding to the C-terminus of SAT bind to the active site of CS and structural data have revealed that the carboxyl­ate group of the C-terminal isoleucine occupies the same space and makes the same interactions as the carboxylate of the α-aminoacrylate catalytic intermediate formed after β-elimination of acetate from the substrate OAS (Rabeh & Cook, 2004 [triangle]; Huang et al., 2005 [triangle]; Francois et al., 2006 [triangle]; Schnell et al., 2007 [triangle]; Salsi, Bayden et al., 2010 [triangle]). A four-amino-acid SAT peptide has been shown to be a competitive inhibitor of Mycobacterium tuberculosis CS with a K i of 5 µM, providing a simple mechanism for complex formation and its dissociation in the presence of elevated levels of OAS (Schnell et al., 2007 [triangle]). Sequence alignments indicate that LmCS contains a SAT-binding motif that was originally identified in Arabidopsis thaliana OAS-TL (AtOAS-TL; Bonner et. al., 2005 [triangle]) and the enzyme can also bind SAT when the proteins are co-expressed in Escherichia coli (Williams et al., 2009 [triangle]).
We undertook a crystallographic and biochemical study of LmCS to investigate the interactions of the enzyme with ligands, including potential inhibitors. Our overall aim was to improve understanding of the enzyme in Leishmania and to provide information that might help to assess the potential of CS as a target for structure-based approaches to develop inhibitors with suitable chemical properties to underpin early-stage drug discovery (Hunter, 2009 [triangle]).
2.1. Protein expression, purification and crystallization  
The recombinant E. coli expression system for LmCS (Williams et al., 2009 [triangle]) was modified by subcloning the LmCS gene from vector pET21a+ into pET15bTEV to allow production of an N-terminally His-tagged protein, which was purified following a standard protocol (Bond et al., 2001 [triangle]). Briefly, the first stage involved nickel ion-affinity chromatography through a 5 ml Ni–NTA column (Qiagen). The product was eluted in a linear imidazole-concentration gradient, which was followed by incubation for 2 h with His-tagged tobacco etch virus (TEV) protease at 303 K prior to dialysis at room temperature against 20 mM Tris–HCl, 150 mM NaCl pH 7.5 for 1 h. The resulting mixture was reapplied onto the Ni–NTA column, which binds the cleaved His tag, the TEV protease and any remaining uncleaved LmCS. The LmCS from which the His tag had been cleaved was present in the flowthrough. Fractions were analyzed using SDS–PAGE and those containing LmCS were pooled. The protein was further purified by size-exclusion chromatography using a Superdex 200 26/60 column (GE Healthcare) equilibrated with 20 mM Tris–HCl, 150 mM NaCl pH 7.5. The final level of LmCS purity was confirmed by matrix-assisted laser desorption/ionization-time of flight mass spectrometry. In preparation for crystallization, the sample was dialyzed into 10 mM Tris–HCl, 100 mM NaCl pH 7.8 and concentrated using a Vivaspin 20 (Sartorius) to provide a stock solution for crystallization. A theoretical extinction coefficient of 16 180 M −1 cm−1 at 280 nm was used to estimate protein concentration (ProtParam; Gasteiger et al., 2005 [triangle]); the theoretical mass of one subunit is estimated as 35.6 kDa.
Crystallization was achieved at 293 K using the hanging-drop vapour-diffusion method with 0.75 µl protein solution at a concentration of 10 mg ml−1 mixed with 0.75 µl reservoir solution consisting of 7.5% PGA-LM (γ-poly-d-glutamic acid low molecular weight) and 19% PEG 3350 (polyethylene glycol average mass 3350) in 0.1 M Tris–HCl pH 7.8. Crystals grew over a period of 2–3 d to approximate dimensions of 50 × 50 × 250 µm and were characterized in-house using a Rigaku HF007 rotating-anode X-ray generator coupled to an R-AXIS IV++ image-plate detector. The presence of PGA-LM and PEG 3350 in the mother liquor allowed the crystals to be cooled to approximately 103 K in a stream of gaseous nitrogen without additional cryoprotection. The crystals were orthorhombic and belonged to space group P212121, with unit-cell parameters a = 48.96, b = 86.3, c = 134.0 Å. Suitable crystals were stored in liquid nitrogen for subsequent data collection at the European Synchrotron Radiation Facility (ESRF), Grenoble, France.
2.2. X-ray data collection, processing, structure solution and refinement  
A well formed sample was selected and diffraction data were measured on beamline ID23-2 at the ESRF using a MAR 225 CCD detector. Data were indexed and integrated using XDS (Kabsch, 2010 [triangle]) and scaled using SCALA (Evans, 2006 [triangle]); the statistics are summarized in Table 1 [triangle]. Diffraction data were collected from a single crystal at a wavelength of 0.87260 Å. The search model for molecular replacement was prepared from the E. coli cysteine synthase B structure (PDB entry 2bhs; Claus et al., 2005 [triangle]). The sequence identity between the search model and LmCS is 39%. Pruning and mutation of this model was carried out using CHAINSAW (Stein, 2008 [triangle]). Molecular replacement was performed in MOLREP (Vagin & Teplyakov, 2010 [triangle]) using a monomer from 2bhs to search for two molecules in the asymmetric unit. A dimer was located, giving a score of 0.396. Refinement was performed in REFMAC5 (Murshudov et al., 2011 [triangle]) and was alternated with rounds of electron-density and difference density map inspection and model manipulation together with water and ligand incorporation using Coot (Emsley & Cowtan, 2004 [triangle]). MolProbity (Chen et al., 2010 [triangle]) was used to investigate model geometry in combination with the validation tools provided in Coot. Final model analysis was performed using JCSG Quality Control Check (http://smb.slac.stanford.edu/jcsg/QC/). Crystallographic statistics are presented in Table 1 [triangle]. Analyses of surface areas and interactions were made using the PISA server (Krissinel & Henrick, 2007 [triangle]) and the figures were prepared with PyMOL (DeLano, 2002 [triangle]). Amino-acid sequence alignments were carried out using the program MUSCLE (Edgar, 2004 [triangle]).
Table 1
Table 1
Data-collection and refinement statistics
2.3. Biochemical analysis  
For biochemical analysis, recombinant LmCS was expressed and purified as a C-terminally His-tagged protein as described previously (Williams et al., 2009 [triangle]). The A. thaliana OAS-TL gene was subcloned from pET3dAtOASTL into pET21 and the recombinant protein AtOAS-TL was expressed and purified in the same way as LmCS.
CS activities were determined at room temperature in 100 µl 200 mM potassium phosphate, 1 mM EDTA, 0.2 mM PLP, 1 mg ml−1 BSA, 3 mM OAS, 2 mM sodium sulfide pH 7.8 with 8 ng LmCS or 12 ng AtOAS-TL. The reaction was started by the addition of sodium sulfide after incubation of all other components for 5 min. Samples were taken before addition of sodium sulfide (0 min) and then every 2 min for 10 min; the cysteine produced was quantified using the azo-dye method described previously (Williams et al., 2009 [triangle]). The rates of cysteine production were linear for 10 min and the specific activities obtained for LmCS and AtOAS-TL were 180 ± 18 and 130 ± 20 µmol min−1 mg−1, respectively. C-terminal SAT peptides are known to bind to the active sites of the plant OAS-TL (Francois et al., 2006 [triangle]) and bacterial OASS enzymes (Huang et al., 2005 [triangle]) and a peptide DFSI based on the SAT sequence is a competitive inhibitor of M. tuberculosis OASS (Schnell et al., 2007 [triangle]). Thus, peptides based on the A. thaliana and L. major SATs and the PGA bound in the crystal of LmCS were tested as inhibitors of the enzyme. Inhibition data were determined by adding various concentrations of different peptides to the pre-incubation mixture and then measuring the enzyme activity. IC50 curves were obtained using GraFit 5 (Erathicus) by plotting the initial rates measured with at least six different concentrations of the peptide. All IC50 values are the means ± standard deviations of three independent determinations, unless otherwise stated. The kinetics of inhibition by the tetrapeptide DYVI were investigated by measuring the initial rates of LmCS without the peptide and then with four different concentrations of peptide (10–100 µM) and six different concentrations of OAS (2.5–20 mM) at a fixed concentration of 2.0 mM sodium sulfide. The type of inhibition was determined from the pattern of the double-reciprocal plots of 1/V against 1/[S] for the different peptide concentrations. The K i was determined by replotting the slopes against the peptide concentration which for competitive inhibition is linear, with the intersect on the x axis representing −K i.
3.1. General comments and overall LmCS structure  
The structure of LmCS was determined to a resolution of 1.8 Å. The biologically active unit, a dimer, constitutes the asymmetric unit (Fig. 1 [triangle]). Subunit A contains residues 3–213 and 241–333, whilst subunit B comprises residues 4–214 and 241–333. A surface loop from residues 214 to 241 is disordered and is therefore missing from the model. The LmCS subunit contains two domains. The smaller domain I is constructed by residues 51–158, which primarily form a four-stranded β-sheet surrounded by four α-helices. The larger domain II comprises residues 21–50 and 159–306. Domain II contains four α-­helices and six β-strands which, together with a β-strand contributed from the partner-subunit domain I, form a seven-membered β-­sheet. In addition, residues 307–333 at the C-terminus form an extended helix–loop–helix structure that stretches across the surface of the partner subunit. This extension is positioned on the opposite face of the dimer to that of the β-sheet intersubunit interaction. These two areas make major contributions to the area of the dimerization interface, which constitutes 22% or 3280 Å2 of the surface area of each subunit.
Figure 1
Figure 1
A ribbon diagram of the LmCS dimer. The helices and strands of subunit A are coloured green and brown, respectively, and in subunit B they are coloured cyan and blue, respectively. The position of the disordered loops A214–A241 and B213– (more ...)
The enzyme purified from the E. coli expression host was cata­lytically active and displayed a yellow colour. Both observations are consistent with the presence of the PLP cofactor. In addition, PLP was added prior to crystallization, seeking to ensure full occupancy. However, the crystals were colourless and there was no electron density to indicate that PLP was present. The affinity of the crystallization agent PGA-LM to bind to LmCS may contribute to the loss of PLP that is observed and the position of a loop formed by residues 181–190 is likely to be a consequence of the absence of the cofactor.
3.2. Binding of γ-poly-d-glutamic acid  
A fragment of the crystallization agent PGA-LM is bound in an ordered fashion to the same region of both subunits of the LmCS dimer. PGA is a pseudopeptide comprising d-glutamic acid residues linked through the amide N atom and the γ-carboxy O atom of an adjacent unit. The use of this compound in protein crystallization was highlighted by Hu et al. (2008 [triangle]).
In subunit A PGA-A comprises five d-glutamic acid moieties (Fig. 2 [triangle]), while PGA-B consists of three d-glutamic acids bound to subunit B (data not shown). The first and second glutamate moieties of PGA-A overlap with the second and third glutamates of PGA-B (data not shown). PGA-A is extended by three additional moieties at one end, while PGA-B has an additional moiety at the other end of the ligand. The interactions between carboxyls from PGA and the side chain and main chain of Thr83 and the main-chain amides of Asn82, Ser274 and Phe273 are common to both binding sites. Also involved in binding PGA-A are Leu312, Ala311 and Ser107 (Fig. 3 [triangle]), while binding of PGA-B also involves Ser78, Ser80, Arg110 and Thr101 (data not shown).
Figure 2
Figure 2
Stereoview of the PGA fragment bound to subunit A. An F oF c OMIT difference density map is shown, where F o are the observed and F c are the calculated structure factors derived from the crystallographic model excluding the contributions from (more ...)
Figure 3
Figure 3
Stereoview of the binding of PGA-A to LmCS. PGA is shown as in Fig. 1 [triangle] and LmCS is shown in green, with N and O atoms of specific side chains coloured blue and red, respectively. Water molecules are shown as cyan spheres and hydrogen-bonding (more ...)
3.3. Comparisons with AtOAS-TL and the PLP-binding site  
LmCS shows a high level of sequence identity to other O-acetyl­serine sulfhydrylases in the PDB. Analysis of the structural conservation using DALI (Holm & Rosenström, 2010 [triangle]) revealed the highest similarity to be to AtOAS-TL (PDB entry 1z7w; Bonner et al., 2005 [triangle]), which shares 47% sequence identity. The superimposition of subunits with LmCS gives an r.m.s.d. of 0.9 Å over 285 Cα residues. Differences between the structures are primarily restricted to loops positioned around the active site. The region from Asp151 to Tyr157 in LmCS forms the start of α7, while in AtOAS-TL this helix is truncated (Fig. 4 [triangle]). The conserved motif QFXNPXN that is present in the vast majority of OAS-TL sequences is replaced by QFATKYN in LmCS; this replacement is also found in L. braziliensis, L. infantum and Trypanosoma cruzi. The first residue of this motif, glutamine, is normally directed towards the active site, although it remains too distant to interact directly with the cofactor. Alteration to the TKY motif causes restructuring of this region, extending the helix that normally follows the motif by an extra two turns. This has two effects. Firstly, the glutamine (Gln152) residue is placed on the opposite face of the helix, far removed from the active site. In addition, the phenylalanine (Phe153) is also positioned away from the entrance to the active site. In LmCS, the placement of these two residues ensures that the active site is considerably widened with respect to that found in orthologues of known structure.
Figure 4
Figure 4
Stereoview of the PGA-ALmCS complex overlaid with a peptide–AtOAS-TL complex. The LmCS structure is shown as in Fig. 3 [triangle], with the locations of α7 and the TKY motif indicated. The model of the AtOAS-TL–peptide (more ...)
The high level of structural conservation between LmCS and the existing structures of O-acetylserine sulfhydrylases is such that the expected binding position for the cofactor PLP can be reliably derived. A lysine (Lys51 in LmCS) forms a Schiff base with PLP, with a conserved asparagine and serine, Asn82 and Ser274 in LmCS, forming hydrogen bonds to PLP. Further residues predicted to orient and hold the PLP in position are Gly186, Thr182, Gly183 and Thr185 of LmCS, which are strictly conserved as Gly181, Thr187, Gly188 and T190 in AtOAS-TL. Structural differences are observed between LmCS and AtOAS-TL in the loop formed by residues 184–190. This loop is glycine-rich; it is therefore likely to be mobile and its position in LmCS is probably influenced by the absence of PLP from the active site.
The binding of PGA may have contributed to the absence of PLP and the unresolved loop between residues 214 and 241 in LmCS (Fig. 4 [triangle]). Again comparing LmCS with AtOAS-TL, it is expected that this loop would fold down and bind into the same groove on the CS surface as that occluded by PGA (Fig. 4 [triangle]). Closer analysis of the position of this loop in AtOAS-TL and comparison with the LmCS structure reveals that PGA interacts with Ser274 (Fig. 3 [triangle]) and supplants the interactions normally expected to form when PLP is bound in the active site (Fig. 4 [triangle]). The position of the side chain of the conserved Arg110 changes considerably as it forms interactions with PGA, whereas normally it would be expected to interact with the highly conserved Gln224 when the 214–241 loop closes over the active site.
3.4. Biochemical analysis  
Following the initial observation of PGA binding in the active site, we tested a (γ-Glu)4 derivative as a potential inhibitor. Despite testing up to a concentration of 500 µM, we were unable to detect any significant inhibition (data not shown). This may relate to the finding, described above, that PGA binding to LmCS does not mimic that of peptides to the active PLP-containing enzyme and may simply be a consequence of the high level of PGA present in the crystallization conditions.
Peptides corresponding to the C-terminus of the L. major and A. thaliana SATs were also tested as inhibitors of LmCS (Table 2 [triangle]). The results obtained for the plant SAT peptide (DYVI), which inhibited LmCS with an IC50 of 7 µM and displayed a similar activity towards A. thaliana OAS-TL, are presented in Fig. 5 [triangle]. Surprisingly, the Leishmania C-terminal peptide GSGI was only a weak inhibitor, with an IC50 of approximately 1.5 mM. Longer peptides derived from the Leishmania SAT sequence had greater activity, with the C-terminal heptapeptide (EGDGSGI) inhibiting LmCS with an IC50 of 270 µM. Similar results were obtained when the Leishmania SAT peptides were tested on AtOAS-TL. These findings are consistent with data from the mutational analysis of SAT from E. coli, which showed that both length and the presence of negatively charged residues were important for complex formation (Zhao et al., 2006 [triangle]). Attempts to cocrystallize LmCS with DYVI were unsuccessful; thus, the binding could not be analysed further.
Table 2
Table 2
Inhibition of LmCS by peptides corresponding to the C-termini of the L. major and A. thaliana SATs
Figure 5
Figure 5
Inhibition of LmCS by the synthetic peptide DYVI. (a) Dose-response curve. Initial rates were determined in reactions containing 3 mM OAS and eight different concentrations of the peptide DYVI (0.1–400 µM). The graph shows (more ...)
Heterologous binding of divergent SAT peptides has been reported previously (Campanini et al., 2005 [triangle]; Francois et al., 2006 [triangle]). The K i of the A. thaliana SAT peptide DYVI for LmCS was determined by measuring the activity with different concentrations of OAS and the peptide at a fixed concentration of sodium sulfide. The double-reciprocal plots showed that the apparent K m increased with increasing peptide concentration, but the V max was not altered and the secondary plot of slope against peptide concentration was linear (data not shown). These results indicate that the heterologous SAT peptide DYVI is a competitive inhibitor of LmCS, with a K i of 4 µM, similar to the inhibition reported for the M. tuberculosis enzyme by its cognate SAT peptide (Schnell et al., 2007 [triangle]).
The carboxylate group of the invariant C-terminal isoleucine provides an anchor for peptide binding and forms hydrogen bonds between key active-site residues that also bind the substrate OAS. These interactions are highly conserved between species (Francois et al., 2006 [triangle]; Schnell et al., 2007 [triangle]). These are in part conserved in the PGA binding through Thr83, but the carboxylate lies too distant from Ser79 to conserve the second interaction (Fig. 3 [triangle]).
Given the importance of the C-terminal isoleucine residue, the free amino acid and certain N-blocked derivatives were also tested for inhibition (Table 2 [triangle]). Isoleucine itself had no activity at 4 mM, whereas two of the N-blocked derivatives inhibited with IC50 values of 250 µM. This increased activity could be the result of the removal of the positively charged amino group or the addition of the hydrophobic blocking group. The carboxybenzyl (CBZ) blocked dipeptide CBZ-l-­valine-isoleucine showed a greatly reduced activity compared with other blocked amino acids, indicating that a valine at this position of the peptide may not be optimal.
The relatively weak activity of the Leishmania SAT peptides for competitive inhibition of LmCS raises questions as to whether CS and SAT could form a functional protein–protein complex in this organism. Differences in the dissociation constants observed for plant and bacterial cysteine synthase complexes (CSCs) were thought to result from differences in the affinity of the SAT C-terminus for the CS active site (Wirtz et al., 2010 [triangle]). However, complex formation in plants and bacteria is now known to involve conformational changes in CS that are not induced by binding of the C-terminal SAT peptide alone (Campanini et al., 2005 [triangle]; Salsi, Campanini et al., 2010 [triangle]; Wirtz et al., 2010 [triangle]; Kumaran et al., 2009 [triangle]). Additional interactions between SAT and CS appear to be required. A sequence motif that was first identified in AtOAS-TL has been implicated in complex formation with SAT by mutagenesis of several conserved basic residues (Lys217, His221 and Lys222) in AtOAS-TL (Bonner et al., 2005 [triangle]), and mutation of the corresponding residues (Lys222, His226 and Lys227) in LmCS also prevented complex formation when CS and SAT were co-expressed in E. coli (Williams et al., 2009 [triangle]). These residues are located on the disordered 213–241 loop in LmCS and are therefore well placed to bind a partner protein at the active site. Although it has been predicted on the basis of molecular modelling that the C-­terminal sequence of Leishmania SAT would not be able to bind to the CS active site (Marciano et al., 2010 [triangle]), our inhibition data, and the conservation of basic residues shown to contribute to complex formation, suggest that L. major SAT and CS could indeed interact. The relatively weak initial interaction with the C-terminal isoleucine might precede conformational changes that support complex formation as observed in the assembly of bacterial CSCs (Salsi, Bayden et al., 2010 [triangle]; Wang & Leyh, 2012 [triangle]). Further work would be required to investigate this aspect of LmCS function, although the presence of PGA in the active site and the loss of PLP cofactor indicate that these crystallization conditions and the crystal form obtained in this study are unsuited to a study of LmCS complexes.
Supplementary Material
PDB reference: cysteine synthase, 4air
Acknowledgments
We thank Professor Rudiger Hell for the plasmid pET3d­AtOASTL. This work was supported by The Wellcome Trust (WT082596 and WT083481 to the University of Dundee and WT085349 and WT061173MA-SM to the University of Glasgow). TR is supported by a Scottish Universities Life Sciences Association studentship. We acknowledge the European Synchrotron Radiation Facility for beam time and excellent staff support.
  • Bond, C. S., White, M. F. & Hunter, W. N. (2001). J. Biol. Chem. 276, 3247–3253. [PubMed]
  • Bonner, E. R., Cahoon, R. E., Knapke, S. M. & Jez, J. M. (2005). J. Biol. Chem. 280, 38803–38813. [PubMed]
  • Campanini, B., Speroni, F., Salsi, E., Cook, P. F., Roderick, S. L., Huang, B., Bettati, S. & Mozzarelli, A. (2005). Protein Sci. 14, 2115–2124. [PubMed]
  • Chen, V. B., Arendall, W. B., Headd, J. J., Keedy, D. A., Immormino, R. M., Kapral, G. J., Murray, L. W., Richardson, J. S. & Richardson, D. C. (2010). Acta Cryst. D66, 12–21. [PMC free article] [PubMed]
  • Claus, M. T., Zocher, G. E., Maier, T. H. & Schulz, G. E. (2005). Biochemistry, 44, 8620–8626. [PubMed]
  • DeLano, W. L. (2002). PyMOL http://www.pymol.org.
  • Edgar, R. C. (2004). Nucleic Acids. Res. 32, 1792–1797. [PMC free article] [PubMed]
  • Emsley, P. & Cowtan, K. (2004). Acta Cryst. D60, 2126–2132. [PubMed]
  • Evans, P. (2006). Acta Cryst. D62, 72–82. [PubMed]
  • Francois, J. A., Kumaran, S. & Jez, J. M. (2006). Plant Cell, 18, 3647–3655. [PubMed]
  • Gasteiger, E., Hoogland, C., Gattiker, A., Duvaud, S., Wilkins, M. R., Appel, R. D. & Bairoch, A. (2005). The Proteomics Protocols Handbook, edited by J. M. Walker, pp. 571–607. Totowa: Humana Press.
  • Holm, L. & Rosenström, P. (2010). Nucleic Acids. Res. 38, W345–W549. [PMC free article] [PubMed]
  • Hu, T.-C., Korczyńska, J., Smith, D. K. & Brzozowski, A. M. (2008). Acta Cryst. D64, 957–963. [PMC free article] [PubMed]
  • Huang, B., Vetting, M. W. & Roderick, S. L. (2005). J. Bacteriol. 187, 3201–3205. [PMC free article] [PubMed]
  • Hunter, W. N. (2009). J. Biol. Chem. 284, 11749–11753. [PMC free article] [PubMed]
  • Kabsch, W. (2010). Acta Cryst. D66, 125–132. [PMC free article] [PubMed]
  • Krauth-Siegel, R. L. & Comini, M. A. (2008). Biochim. Biophys. Acta, 1780, 1236–1248. [PubMed]
  • Krissinel, E. & Henrick, K. (2007). J. Mol. Biol. 372, 774–797. [PubMed]
  • Kumaran, S., Yi, H., Krishnan, H. B. & Jez, J. M. (2009). J. Biol. Chem. 284, 10268–10275. [PubMed]
  • Marciano, D., Santana, M., Mantilla, B. S., Silber, A. M., Marino-Buslje, C. & Nowicki, C. (2010). Mol. Biochem. Parasitol. 173, 170–174. [PubMed]
  • Murshudov, G. N., Skubák, P., Lebedev, A. A., Pannu, N. S., Steiner, R. A., Nicholls, R. A., Winn, M. D., Long, F. & Vagin, A. A. (2011). Acta Cryst. D67, 355–367. [PMC free article] [PubMed]
  • Nozaki, T., Ali, V. & Tokoro, M. (2005). Adv. Parasitol. 60, 1–99. [PubMed]
  • Rabeh, W. M. & Cook, P. F. (2004). J. Biol. Chem. 279, 26803–26806. [PubMed]
  • Salsi, E., Bayden, A. S., Spyrakis, F., Amadasi, A., Campanini, B., Bettati, S., Dodatko, T., Cozzini, P., Kellog, G. E., Cook, P. F., Roderick, S. L. & Mozzarelli, A. (2010). J. Med. Chem. 53, 345–356. [PMC free article] [PubMed]
  • Salsi, E., Campanini, B., Bettati, S., Raboni, S., Roderick, S. L., Cook, P. F. & Mozzarelli, A. (2010). J. Biol. Chem. 285, 12813–12822. [PubMed]
  • Schnell, R., Oehlmann, W., Singh, M. & Schneider, G. (2007). J. Biol. Chem. 282, 23473–23481. [PubMed]
  • Stein, N. (2008). J. Appl. Cryst. 41, 641–643.
  • Vagin, A. & Teplyakov, A. (2010). Acta Cryst. D66, 22–25. [PubMed]
  • Wang, T. & Leyh, T. S. (2012). J. Biol. Chem. 287, 4360–4367. [PubMed]
  • Williams, R. A., Westrop, G. D. & Coombs, G. H. (2009). Biochem. J. 420, 451–462. [PubMed]
  • Wirtz, M., Birke, H., Heeg, C., Müller, C., Hosp, F., Throm, C., König, S., Feldman-Salit, A., Rippe, K., Petersen, G., Wade, R. C., Rybin, V., Scheffzek, K. & Hell, R. (2010). J. Biol. Chem. 285, 32810–32817. [PubMed]
  • Zhao, C., Moriga, Y., Feng, B., Kumada, Y., Imanaka, H., Imamura, K. & Nakanishi, K. (2006). Biochem. Biophys. Res. Commun. 341, 911–916. [PubMed]
Articles from Acta Crystallographica Section F: Structural Biology and Crystallization Communications are provided here courtesy of
International Union of Crystallography