Search tips
Search criteria 


Logo of actafjournal home pagethis articleInternational Union of Crystallographysearchsubscribearticle submission
Acta Crystallogr Sect F Struct Biol Cryst Commun. 2008 August 1; 64(Pt 8): 760–763.
Published online 2008 July 31. doi:  10.1107/S1744309108021490
PMCID: PMC2494972

Crystallization and preliminary crystallographic analysis of mannosyl-3-phosphoglycerate synthase from Rubrobacter xylanophilus


Rubrobacter xylanophilus is the only Gram-positive bacterium known to synthesize the compatible solute mannosylglycerate (MG), which is commonly found in hyperthermophilic archaea and some thermophilic bacteria. Unlike the salt-dependent pattern of accumulation observed in (hyper)thermophiles, in R. xylanophilus MG accumulates constitutively. The synthesis of MG in R. xylanophilus was tracked from GDP-mannose and 3-phosphoglycerate, but the genome sequence of the organism failed to reveal any of the genes known to be involved in this pathway. The native enzyme was purified and its N-terminal sequence was used to identify the corresponding gene (mpgS) in the genome of R. xylanophilus. The gene encodes a highly divergent mannosyl-3-phospho­glycerate synthase (MpgS) without relevant sequence homology to known mannosylphosphoglycerate synthases. In order to understand the specificity and enzymatic mechanism of this novel enzyme, it was expressed in Escherichia coli, purified and crystallized. The crystals thus obtained belonged to the hexagonal space group P6522 and contained two protein molecules per asymmetric unit. The structure was solved by SIRAS using a mercury derivative.

Keywords: mannosylglycerate, Rubrobacter xylanophilus, compatible solutes, GDP-mannose, 3-phosphoglycerate

1. Introduction

The radiation-resistant bacterium Rubrobacter xylanophilus is moderately halotolerant and has an optimum growth temperature of about 333 K (Carreto et al., 1996 [triangle]). It accumulates trehalose and mannosylglycerate (MG) intracellularly under both normal and stress growth conditions (Empadinhas et al., 2007 [triangle]). Two pathways for the synthesis of MG have so far been identified: one involves the direct conversion of GDP-mannose and d-glycerate into MG by mannosylglycerate synthase (MgS), while the other comprises the consecutive synthesis and dephosphorylation of mannosyl-3-phosphoglycerate (MPG) by MPG synthase (MpgS; EC and MPG phosphatase (MpgP; EC from GDP-mannose and 3-phosphoglycerate (3-PGA) (Empadinhas et al., 2001 [triangle]; Martins et al., 1999 [triangle]).

Glucosylglycerate (GG), a solute structurally related to MG, has been detected in bacteria and archaea in minor amounts and has been shown to serve in the osmotic adaptation of Erwinia chrysanthemi in nitrogen-depleted media (Goude et al., 2004 [triangle]). Two pathways for the synthesis of GG have so far been elucidated: a single-step pathway and a two-step mechanism via glucosyl-3-phosphoglycerate (GPG), mechanistically similar to those for the synthesis of MG (Costa et al., 2006 [triangle]; Fernandes et al., 2007 [triangle]). GG has also been detected in the polar head of a glycolipid from a species of Nocardia and in methylglucose polysaccharides from Mycobacterium sp. (Kamisango et al., 1987 [triangle]; Tuffal et al., 1998 [triangle]). A highly divergent GPG synthase (GpgS) has been recently characterized in M. bovis and in M. smegmatis, where it has been proposed to synthesize GPG as a primer for the assembly of unique GG-containing methylglucose polysaccharides (Empadinhas et al., 2008 [triangle]; Kamisango et al., 1987 [triangle]; Tuffal et al., 1998 [triangle]). The mycobacterial GpgS gene has close homologues in many Actinobacteria and, coincidently, the R. xylanophilus homologue is the mpgS gene that has now been identified. This ancient enzyme might represent a close relative of the common ancestor of strict MpgSs and GpgSs preceding the divergence of these two activities. The closest R. xylanophilus MpgS homologue of known three-dimensional structure is the spore-coat-forming protein SpSA from Bacillus subtilis (11% identity), a monomeric glycosyl transferase belonging to GT family 2 and possessing a GT-A-like fold (Charnock & Davies, 1999 [triangle]). Structural characterization of this novel enzyme by X-ray crystallography should provide further insights towards the clarification of its specificity and constitute a framework for a detailed structural comparison with homofunctional GpgSs. Here, we report the expression, purification, crystallization and preliminary crystallo­graphic analysis of the MpgS from R. xylanophilus.

2. Materials and methods

2.1. Purification of native MpgS

R. xylanophilus DSM 9941 cells (Deutsche Sammlung von Mikroorganismen und Zellkulturen, Braunschweig, Germany) were grown at 333 K in Thermus medium pH 7.0 (Williams & da Costa, 1992 [triangle]). Cells were harvested during the late exponential phase of growth, suspended in 20 mM Tris–HCl pH 7.6 containing 5 mM MgCl2, 2 mg ml−1 DNAse I and a protease-inhibitor cocktail (Roche, Germany), disrupted with a French press cell and centrifuged to remove debris. The supernatant was dialyzed against 20 mM Tris–HCl pH 7.6 (buffer A) and loaded onto two sequential Q-Sepharose FF columns (Hi-Load 16/10) equilibrated with the same buffer. Elution was carried out with linear NaCl gradients (0.0–1.0 M) and the enzyme activity was determined as described previously (Empadinhas et al., 2001 [triangle], 2008 [triangle]). Active fractions were concentrated, dialyzed against buffer A and further purified by ion-exchange chromatography on a Mono-Q column using the same buffer system. The purest sample was blotted onto a PVDF membrane and subjected to N-terminal amino-acid sequencing (Microchemical Facility, Emory University School of Medicine, Georgia, USA). The N-terminal protein sequences obtained were used to identify the MpgS gene in the R. xylanophilus genome sequence (

2.1.1. Cloning and functional overexpression of mpgS in Escherichia coli

Specific primers (RuMG1, 5′-CATGAATTCATGAGTACTTATCATGAGAG-3′, and RuMG2, 5′-CATAAGCTTCTACCTTACCCTCAGCACCTC-3′) were designed and used to amplify the mpgS gene (GenBank accession No. EU847586) by PCR using 100 ng R. xylanophilus chromosomal DNA (Rainey et al., 1996 [triangle]) as a template. The amplified fragment was cloned into the pGEM T-­Easy vector (Promega) for sequencing purposes. The mpgS ORF was cloned between the EcoRI and HindIII sites of pET30a (Novagen) to allow the production of an N-terminal His-tagged protein. The expression construct encodes all 335 residues of mature MpgS, preceded by 52 residues forming the affinity tag (MHHHH­HHSSGLVPRGSGMKETAAAKFERQHMDSPDLGTDDDDKA­MADIGSEF). Expression in E. coli BL21 (DE3) cells was induced with IPTG (final concentration 1 mM) at mid-exponential growth (OD600 = 0.8) and allowed to proceed for 6–8 h at 303 K. The cells were harvested and the crude extract prepared as described in §2.1.

2.1.2. Purification of recombinant MpgS

The His-tagged MpgS was purified by immobilized metal-affinity chromatography on an Ni-Sepharose column (His-Prep FF 16/10) equilibrated with 20 mM sodium phosphate buffer pH 7.4, 0.5 M NaCl, 20 mM imidazole. Elution was carried out with a linear gradient of imidazole (0.05–0.5 M) and MpgS activity was detected as described previously (Empadinhas et al., 2001 [triangle], 2008 [triangle]). The selected fractions were dialyzed against 20 mM Tris–HCl pH 8.0 and further purified by anion-exchange chromatograpy (Q-Sepharose FF). The purity of the samples was determined by SDS–PAGE.

2.2. Crystallization, data collection and processing

2.2.1. MpgS crystallization

Initial crystallization conditions were identified in sitting-drop trials using commercial sparse-matrix crystallization screens (Hampton Research). After optimization, the best native MpgS crystals were obtained at 293 K using the hanging-drop vapour-diffusion method from drops consisting of 4 µl protein solution (16 mg ml−1 in 10 mM Tris–HCl pH 7.5, 1 mM MgCl2) and 2 µl precipitant solution (0.1 M MES pH 6.0, 2.0 M NaCl, 0.1 M NaH2PO4 and 0.1 M KH2PO4) equilibrated against a 500 µl reservoir. Crystals of the MpgS–GDP–mannose ternary complex were obtained from a 1:10:10 protein:GDP:mannose mixture pre-incubated at 277 K for 1 h using the crystallization conditions for the native protein. To obtain the mercury derivative, crystals of native MpgS were soaked for 12 h in a solution of p-chloromercuribenzoic acid (0.1 M MES buffer pH 6.0, 2.0 M NaCl, 0.1 M NaH2PO4, 0.1 M KH2PO4, 10 mM p-chloro­mercuribenzoic acid). The cryoprotection protocol involved the sequential transfer of crystals into drops of 0.15 M MES pH 6.0, 2.4 M NaCl, 0.15 M NaH2PO4 and 0.15 M KH2PO4 supplemented with increasing concentrations of glycerol [15, 20 and 25%(v/v)]. Crystals were finally cryocooled and stored in liquid nitrogen prior to X-ray data collection.

2.2.2. Data collection and processing

X-ray diffraction data for native MpgS and mercury-labelled MpgS were collected on beamline ID14-EH3 of the European Synchrotron Radiation Facility (ESRF, Grenoble, France). For the native protein, a data set extending to 2.20 Å resolution was collected on an ADSC Q4R detector from a single crystal at 100 K in 0.5° oscillation steps over a range of 150°. For the mercury derivative, a data set extending to 3.05 Å resolution was collected using a single crystal in 1° oscillation steps over a range of 120°. For the ternary complex with GDP and mannose, a data set extending to 2.80 Å resolution was collected at 100 K from a single crystal in 0.5° oscillation steps over a range of 135° using an ADSC 210 detector on the macromolecular crystallography beamline ID14-EH1 of the ESRF (Grenoble, France). Diffraction data sets were processed with MOSFLM (Leslie, 1991 [triangle]) and SCALA from the CCP4 suite (Collaborative Computational Project, Number 4, 1994 [triangle]).

2.3. Structure solution

The structure was solved by the single isomorphous replacement with anomalous scattering (SIRAS) method. Using autoSHARP (Vonrhein et al., 2007 [triangle]) and data from the native crystal and the mercury derivative, two mercury sites were successfully located. Phases were further improved and extended to the diffraction limit of the native data by density modification and twofold averaging using SOLOMON (Abrahams & Leslie, 1996 [triangle]) and then used for automatic model building in ARP/wARP (Perrakis et al., 1999 [triangle]).

3. Results and discussion

3.1. Protein characterization and recombinant expression

Native MpgS was partially purified in four chromatographic steps. The purest preparation contained four bands on SDS–PAGE, the N-­terminal sequences of which were determined (N. Empadinhas & M. S. da Costa, unpublished results). These sequences allowed the identification of four distinct ORFs in the R. xylanophilus genome, one of which (Rxyl_2312) coded for a 37.3 kDa putative family 2 glycosyltransferase, a likely candidate for MpgS activity.

Cloning and expression of Rxyl_2312 in E. coli produced clones whose protein extracts showed extra bands of ~43 kDa on SDS–PAGE (consistent with the molecular weight of the fusion construct) and catalyzed MPG synthesis, while extracts from E. coli with the empty vector did not. Heat-treatment (333 K, 20 min) of independent E. coli extracts containing His-tagged MpgS resulted in extensive purification of the recombinant enzyme and further purification by FPLC yielded pure protein as judged by SDS–PAGE (Fig. 1 [triangle]). The recombinant His-tagged protein eluted from the gel-filtration column with an apparent molecular weight of approximately 95 kDa, suggesting that it is dimeric in solution, which was confirmed by DLS (data not shown). Biochemical assays to determine the enzymatic activity and specificity of MpgS are currently under way.

Figure 1
Coomassie Blue-stained 12.5% SDS–PAGE of the purified recombinant MpgS from R. xylanophilus used for crystallization trials.

3.2. Crystallization of MpgS

Crystals of native MpgS were hexagonal bipyramidal with maximum dimensions of 0.6 × 0.25 × 0.3 mm (Fig. 2 [triangle]) and diffracted to 2.2 Å resolution (Fig. 3 [triangle]). The crystals were extremely fragile and manipulation for cryoprotection often resulted in reduced diffraction quality. In order to obtain improved diffraction patterns, quick transfer (less than 5 s) between the different cryoprotecting solutions containing increasing concentrations of glycerol was critical.

Figure 2
Single crystals of native MpgS from R. xylanophilus belonging to the hexagonal space group P6522.
Figure 3
X-ray diffraction pattern of an MpgS crystal recorded on the ESRF ID14-EH3 beamline. The external circumference corresponds to 2.09 Å resolution and the resolution at the corner of the image is 1.59 Å. A magnification of ...

The data-collection and phasing statistics are summarized in Table 1 [triangle]. The crystals belong to the hexagonal space group P6522, with unit-cell parameters a = b = 108.9, c = 311.7 Å. Assuming the presence of two monomers per asymmetric unit, the calculated Matthews coefficient is 3.10 Å3 Da−1, which corresponds to a solvent content of 60.4% (Matthews, 1968 [triangle]). This relatively high solvent content explains the inherent mechanical fragility of the MpgS crystals.

Table 1
Statistics of diffraction data collection

3.3. Structure solution

The structure was solved by the single isomorphous replacement with anomalous scattering (SIRAS) method using autoSHARP (Vonrhein et al., 2007 [triangle]). The hexagonal space-group ambiguity was solved by analyzing the ‘map contrast’ and ‘map connectivity’ statistics calculated for space groups P6522 and P6122. The statistics and final electron-density maps were clearly better for P6522 than for the alternative P6122 space group. Given the relatively high solvent content of the crystals (60.4%), solvent flattening was highly effective at improving the quality of the maps, which was further helped by twofold averaging and phase extension to the resolution limit of the native data. The experimentally phased, solvent-flattened and twofold-averaged electron-density maps were of good quality and a significant portion of the model (583 of 774 residues) could be traced automatically with ARP/wARP (Perrakis et al., 1999 [triangle]). The model is currently being refined and revealed a dimeric arrangement of the enzyme. The three-dimensional structure of R. xylanophilus MpgS will provide the basis for further studies aiming at understanding the structure and activity of this novel enzyme.


We acknowledge the ESRF for provision of synchrotron-radiation facilities and thank the ESRF staff for help with data collection at beamlines ID14-EH3 and ID14-EH1. We gratefully acknowledge funding from Fundação para a Ciência e Tecnologia, Portugal (POCI/BIA-MIC/56511/2004 and PTDC/SAU-MII/70634/2006).


  • Abrahams, J. P. & Leslie, A. G. W. (1996). Acta Cryst. D52, 30–42. [PubMed]
  • Carreto, L., Wait, R., Nobre, M. F. & da Costa, M. S. (1996). J. Bacteriol.178, 6479–6486. [PMC free article] [PubMed]
  • Charnock, S. J. & Davies, G. J. (1999). Biochemistry, 38, 6380–6385. [PubMed]
  • Collaborative Computational Project, Number 4 (1994). Acta Cryst. D50, 760–763. [PubMed]
  • Costa, J., Empadinhas, N., Goncalves, L., Lamosa, P., Santos, H. & da Costa, M. S. (2006). J. Bacteriol.188, 1022–1030. [PMC free article] [PubMed]
  • Empadinhas, N., Albuquerque, L., Mendes, V., Macedo-Ribeiro, S. & da Costa, M. S. (2008). FEMS Microbiol. Lett.280, 195–202. [PubMed]
  • Empadinhas, N., Marugg, J. D., Borges, N., Santos, H. & da Costa, M. S. (2001). J. Biol. Chem.276, 43580–43588. [PubMed]
  • Empadinhas, N., Mendes, V., Simoes, C., Santos, M. S., Mingote, A., Lamosa, P., Santos, H. & Costa, M. S. (2007). Extremophiles, 11, 667–673. [PubMed]
  • Fernandes, C., Empadinhas, N. & da Costa, M. S. (2007). J. Bacteriol.189, 4014–4019. [PMC free article] [PubMed]
  • Goude, R., Renaud, S., Bonnassie, S., Bernard, T. & Blanco, C. (2004). Appl. Environ. Microbiol.70, 6535–6541. [PMC free article] [PubMed]
  • Kamisango, K., Dell, A. & Ballou, C. E. (1987). J. Biol. Chem.262, 4580–4586. [PubMed]
  • Leslie, A. (1991). Crystallographic Computing 5, edited by D. Moras, A. D. Podjarny & J. C. Thierry, pp. 27–38. Oxford University Press.
  • Martins, L. O., Empadinhas, N., Marugg, J. D., Miguel, C., Ferreira, C., da Costa, M. S. & Santos, H. (1999). J. Biol. Chem.274, 35407–35414. [PubMed]
  • Matthews, B. W. (1968). J. Mol. Biol.33, 491–497. [PubMed]
  • Perrakis, A., Morris, R. & Lamzin, V. S. (1999). Nature Struct. Biol.6, 458–463. [PubMed]
  • Rainey, F. A., Ward-Rainey, N., Kroppenstedt, R. M. & Stackebrandt, E. (1996). Int. J. Syst. Bacteriol.46, 1088–1092. [PubMed]
  • Tuffal, G., Albigot, R., Riviere, M. & Puzo, G. (1998). Glycobiology, 8, 675–684. [PubMed]
  • Vonrhein, C., Blanc, E., Roversi, P. & Bricogne, G. (2007). Methods Mol. Biol.364, 215–230. [PubMed]
  • Williams, R. A. D. & da Costa, M. S. (1992). The Prokaryotes, edited by A. Balows, H. G. Trüper, M. Dworkin, W. Harder & K. H. Schleifer, pp. 3745–3753. New York: Springer.

Articles from Acta Crystallographica Section F: Structural Biology and Crystallization Communications are provided here courtesy of International Union of Crystallography