1 Department of Medical Microbiology and Immunology, 1-63 Medical Sciences Building, University of Alberta, Edmonton, Alberta, Canada T6G 2R3
2 National Microbiology Laboratory, Health Canada, Winnipeg, Manitoba, Canada R3E 3R2
3 Instituto de Biologia Experimental, Facultad de Ciencias, Universidad Central de Venezuela, Caracas, Venezuela
Correspondence
Diane E. Taylor
diane.taylor{at}ualberta.ca
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ABSTRACT |
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INTRODUCTION |
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Coupling proteins are polytopic, inner-membrane proteins containing two transmembrane regions near the N-terminus of the proteins; the N- and C-terminal regions of the proteins are located within the cytoplasm, and a periplasmic region separates the two transmembrane domains (Das & Xie, 1998; Gomis-Ruth et al., 2001
; Kumar & Das, 2002
; Lee et al., 1999
; Okamoto et al., 1991
; Schroder et al., 2002
). The 3D structure of the cytoplasmic domain of TrwB, a coupling protein encoded on the incompatibility (Inc) group W plasmid R388, revealed a hexameric, spherical particle with a central channel that ranges in diameter from 78 Å (0·70·8 nm) at the cytoplasmic side to 22 Å at the membrane end (Gomis-Ruth et al., 2001
). Biochemical analysis of coupling proteins from R388, RP4 (IncP
) and F (IncFI) plasmids have revealed that this family of proteins are able to bind in a non-specific fashion to DNA (Hormaeche et al., 2002
; Moncalian et al., 1999
; Schroder et al., 2002
). In addition, coupling proteins have conserved motifs such as the Walker-type nucleoside triphosphate (NTP)-binding domains. Recent analysis of TrwB has revealed that this coupling protein is a DNA-dependent ATPase (Tato et al., 2005
). Mutational analyses of the Walker motifs of TraG, the coupling protein from RP4, indicated that the Lys and Asp residues, at positions 187 and 449 of RP4, were essential for conjugation of the IncP plasmid (Balzer et al., 1994
).
The most recent advance in the study of coupling proteins has been the identification of the Mpf component to which the coupling protein binds. The coupling proteins TraG and TrwB from the R27 and R388 plasmids, respectively, were both independently determined to interact with the VirB10-like proteins, TrhB and TrwE, from R27 and R388 (Gilmour et al., 2003; Llosa et al., 2003
). In the Ti plasmid of Agrobacterium tumefaciens, VirB10 is a well-conserved T4SS component and it has been recently proposed to be the ATP energy sensor of the T4SS (Cascales & Christie, 2004a
).
The cellular location of the coupling protein has only been demonstrated in A. tumefaciens. VirD4 was found to associate with the poles of A. tumefaciens, and this polar localization was determined to occur in the absence of other essential conjugation proteins (Kumar & Das, 2002). Subsequent localization experiments with A. tumefaciens revealed that a T4SS protein, VirB6, co-localized with VirD4 at the poles of the cell (Jakubowski et al., 2004
; Judd et al., 2005
). In contrast, a GFP fusion to the T4SS protein TrhC from R27 revealed that this VirB4 homologue was found at random positions around the periphery of the cell (Gilmour et al., 2001
). The fluorescent foci formed when TrhC was labelled with GFP resulted in membrane-associated protein complexes which required a number of R27 T4SS proteins (Gilmour & Taylor, 2004
).
Our goal was to characterize the coupling protein TraG from the IncHI1 resistance plasmid R27, originally isolated from Salmonella enterica serovar Typhi (Lawley et al., 2002; Sherburne et al., 2000
). The IncHI plasmids are unique in that conjugative transfer is optimal at 30 °C, and at 37 °C transfer is significantly reduced (Taylor & Levine, 1980
). We have determined that traG expression is reduced at 37 °C, in comparison with the expression profile observed at 30 °C. Site-specific mutagenesis within traG demonstrated that well-conserved residues in the NTP-binding Walker regions are essential for R27 conjugation. In addition, bacterial two-hybrid and immunoprecipitation interaction data determined that substitutions in the four periplasmic-spanning residues of TraG prevented an interaction with the VirB10 homologue, TrhB. Notably, these periplasmic substitutions did not completely abolish conjugative transfer of the R27 plasmid. Finally, immunofluorescence microscopy was used to determine the subcellular location of TraG. In contrast to the VirD4 polar localization in A. tumefaciens, TraG formed fluorescent foci at random positions in the membrane of Escherichia coli. The position and number of foci formed by TraG are similar to the distribution of TrhC within the cell.
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METHODS |
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RT-PCR.
For RT-PCR amplification of traG transcripts, 2 µg total RNA was used as a template. RNA was retrotranscribed into cDNA utilizing the SuperScriptII RT (Invitrogen) with the random hexamers included in the kit. A 1/10 dilution of each retrotranscription was subjected to PCR using the primer pairs specific for the two adjacent genes (Table 2). A negative control containing no template and a negative control with total RNA that had not been retrotranscribed were included in each PCR reaction. A positive control of R27 template DNA was prepared for each primer pair and PCR reactions generated products of predicted sizes. The E. coli pfkA housekeeping gene, which encodes phosphofructokinase, was included as a positive control for the bacterial transcripts. Amplified products were resolved on a 1 % agarose gel stained with ethidium bromide. RT-PCR amplifications were performed at least twice with total RNA preparations obtained from a minimum of three independent extractions. Similar results were obtained in all experiments.
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Insertional mutagenesis of traG on drR27.
A gene disruption in traG was created using the E. coli recombination system, as described previously (Lawley et al., 2002; Yu et al., 2000
). A trimethoprim-resistance dihydrofolate reductase cassette, dhfrIIc, was inserted into traG of R27. A linear DNA construct was created using PCR primers that amplified dhfrIIc and also contained
40 bp terminal arms homologous to traG at positions 528563 and 15451585 (Table 2
). Presumptive traG mutants were screened using PCR to detect a 237 bp size increase in traG.
Conjugation.
Complementation experiments with R27 were performed as described previously (Lawley et al., 2002; Taylor & Levine, 1980
). Briefly, DY330R cells containing drR27 plasmid or an R27 plasmid containing a mutation within the coupling protein gene, traG, were grown at 28 °C. DY330N recipient cells were also grown at 28 °C. pDT3152, an R27 plasmid containing a traG mutation, was complemented by transforming donor cells with pJEG217 or variants. Upon reaching an OD600 of 0·50·7, donor cells containing the complementation constructs were induced for 1 h with IPTG at a final concentration of 0·4 mM. Donor and recipient cells were incubated for 16 h at 28 °C. Transconjugants and donors were then plated on selective media after serial dilutions. The transmission frequency was expressed as transconjugants per donor.
Immunofluorescence microscopy.
E. coli cells containing pJEG217 were processed for immunofluorescence microscopy according to Kumar & Das (2002). Briefly, E. coli cells were grown at 30 °C, unless stated otherwise, to an OD600 of 0·50·7, then treated for 1 h with IPTG at a final concentration of 0·4 mM. After washing with phosphate-buffered saline (PBS), cells were fixed with 4 % paraformaldehyde for 1 h on ice. The cells were washed three times with PBS and resuspended in 300 µl 25 mM Tris/HCl, 1·8 % glucose and 10 mM EDTA pH 8·0. The resuspension was mixed for 10 min on ice with lysozyme at a final concentration of 2 mg ml1. Aliquots (50 µl) of the treated cells were spotted onto wells of poly-L-lysine-coated slides and allowed to adhere for 15 min at room temperature. Excess liquid was aspirated from the slides, and the dry slides were washed 10 times with PBS before the addition of 2 % bovine serum albumin (BSA) blocking solution. Slides were incubated with BSA at 37 °C for 30 min, prior to the addition of mouse anti-His antibodies (Invitrogen) and incubation at 4 °C overnight. After washing 10 times with PBS, the slides were incubated with goat anti-mouse antibody conjugated to Alexa Fluor 488 for 1 h at room temperature. After further washing with PBS, the slides were mounted with an antifade mounting medium (p-phenylenediamine in 40 % glycerol). Images were collected with a Leica DMI 6000 B microscope equipped with a Hamamatsu Orca ER camera. Image analysis was performed using OpenLab 4.0.2 software.
Bacterial two-hybrid (BTH) system.
The conjugative proteins were fused to the catalytic domain of adenylate cyclase from Bordetella pertussis via cloning into the BTH vectors, pKT25 and pUT18C (Karimova et al., 1998). Plasmids encoding fused proteins were co-transformed into competent BTH101 cells and plated on LB plates with ampicillin, kanamycin and X-Gal at a final concentration of 100 µg ml1. Cultures were grown at 30 °C for 4048 h or until the colonies expressing the leucine-zipper-positive control became dark blue in colour due to the degradation of the chromogenic substrate X-Gal. For each interaction, two colonies were streaked on to the above medium and grown at 30 °C for 16 h. These colonies were used to inoculate a 20 ml volume of LB with ampicillin and kanamycin selection and grown at 30 °C for 16 h at 250 r.p.m. The
-galactosidase activity of each culture was measured using the Miller assay (Miller, 1972
).
Immunoprecipitation.
Immunoprecipitation was performed as described previously with minor modifications (Gilmour et al., 2003). Briefly, DH5
cells containing pKT25-TraG or pKT25-TraG : S4 were co-transformed with pMS119EH-trhBFLAG. Cells were induced at mid-exponential growth phase (OD600 0·50·7) with 0·4 mM IPTG for 1 h before lysis. Harvested cells were resuspended in 1 ml lysis buffer [PBS pH 7·4, 150 mM NaCl, 1 % NP-40, 7·15 % sucrose, 0·2 mg lysozyme ml1, 1x anti-protease cocktail (Complete; Boehringer Mannheim)] freezethawed three times and sonicated for 3 min (30 s pulses, 10 s breaks, Fisher 300 sonicator). The cell lysates were mixed with 40 µl ANTI-FLAG M2-agarose affinity gel (Sigma). The affinity gel was pre-blocked with 5 % BSA for 16 h. The cellular lysates and affinity gel were rotated at 4 °C for 16 h. The gel was then washed three times with 1 ml lysis buffer. Proteins were eluted from the gel by boiling in Laemmli sample buffer+DTT and resolved on a 10 % SDS-PAG, transferred to nitrocellulose and blocked with 10 % (w/v) skimmed milk powder, 0·1 % Tween 20 in PBS. A primary antibody of anti-adenylate cyclase [rabbit serum #L24023, specific for the catalytic domain (D. Ladant)] was applied to the nitrocellulose, washed, and a secondary antibody (anti-rabbit HRP, Sigma) was applied for 1 h.
Web-based computer programs.
PSI-BLAST (http://www.ncbi.nlm.nih.gov/blast/); CLUSTALW (Gonnet matrix; gap penalty 10, extension penalty 0·2; http://www.ebi.ac.uk/clustalw/) and TMHMM (http://www.cbs.dtu.dk/services/TMHMM-2.0/) were used.
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RESULTS |
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The amplification of RNA from both traItraG and traGorf118 was markedly different when an RNA template was extracted from cells grown at 30 °C or 37 °C (Fig. 1b). The RT-PCR is only a semi-quantitative technique; however, the difference in the transcript levels indicates that the effect of temperature on conjugation results from regulation at the transcriptional level. The 1-8 and 1-9 primer sets indicate that there is transcriptional activity of the H operon at both 30 °C and 37 °C. The transcript levels of pfkA, the RT-PCR control, were similar when the template was RNA extracted from cells grown at 30 °C or 37 °C (Fig. 1b
).
Generation of NTP-binding motif mutations in traG
We have previously cloned traG into the expression vector pMS119EH, with a His6 tag on the 3' end of the gene, to form the construct pJEG217 (Table 1). The His-tagged coupling protein contains a Walker A motif (GxxGxGKS/T) and a Walker B motif (hhhhDE; where h is a hydrophobic residue) commencing at amino acid positions 205 and 506, respectively (Fig. 2a, b
) (Schneider & Hunke, 1998
). The Walker motifs are involved with NTP binding and hydrolysis, and these motifs represent the region with the highest level of homology among coupling proteins (Fig. 2a, b
) (Schneider & Hunke, 1998
). Site-specific mutagenesis was performed on the Walker A and Walker B motifs of pJEG217, and the resultant plasmid constructs were transformed into DY330R cells harbouring pDT3152 (drR27 with a traG mutation). The residues that were substituted for the well-conserved Gly and Lys residues (GK) of Walker A, and the Asp and Glu residues (DE) of Walker B, were selected using a matrix designed for creating safe substitutions' that minimized protein instability (Fig. 2c
) (Bordo & Argos, 1991
). Within the Walker A region, the small, non-polar Gly was substituted with the negatively charged, polar Asp (G210D). The positively charged, polar Lys was replaced with the large, positively charged Arg residue (K211R). A complete deletion of the Walker A subregion Gly-Lys (
GK) was also created in pJEG217. Within the Walker B region, the Asp residue with an acidic side chain was substituted with the small, non-polar Ser (D510S). The negatively charged, polar Glu residue was replaced with the positively charged, polar Lys (E511K). Finally, the Walker B subregion (
DE) was deleted from pJEG217.
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Production and stability of TraGHis6 containing mutations within the Walker A and B regions
The inability of pJEG217 derivatives containing Walker A or B mutations to complement pDT3152 could be a result of a mutation causing instability in the mutant coupling protein. To ensure that the substitutions and deletions within the Walker A or B motifs of the R27 coupling protein did not affect protein expression or stability, the steady-state levels of WT and mutant proteins were compared by semiquantitative immunoblot analyses. When equivalent amounts of protein were loaded in an SDS-PAG and transferred to a nitrocellulose membrane, an anti-His antibody revealed similar levels of protein expression for four pJEG217 mutants, G210D, GK, D510S and E511K (Fig. 3
). Degradation products were detected in the cell extract of cells harbouring pJEG217; however, three mutants,
GK, D510S and E511K, appeared to contain significantly higher levels of degradation products. Although the expression levels of these three pJEG217 variants were similar to those of WT pJEG217, the mutations may have slightly altered the stability of the coupling protein. There was a partial reduction in the amount of coupling protein detected in the cell extract of DY330R containing pDT3152 and pJEG217 with a K211R mutation (Fig. 3
). Notably, the deletion of the Asp and Glu residues (
DE) of the Walker B region of TraG in pJEG217 created an unstable protein, as there was no detectable protein in the immunoblot (Fig. 3
).
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To verify the data from the in vivo BTH experiments, in which substitutions in the periplasmic domain of TraG abrogated an interaction with TrhB, we attempted to precipitate a complex of epitope-tagged TrhB and TraG : S4. Whereas TrhB containing a C-terminal FLAG epitope (Asp-Tyr-Lys-Asp-Asp-Asp-Asp-Lys) precipitated TraGAC, the anti-adenylate cyclase antibody did not detect TraG : S4AC precipitated by TrhBFLAG (Fig. 6). This biochemical analysis confirms that the periplasmic residues of the R27 coupling protein are essential for a successful interaction with the Mpf protein TrhB.
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To determine if TraG localized to the same position as these Mpf complexes, we used immunofluorescence microscopy to probe for the location of TraGHis6 proteins. Interestingly, these studies revealed that DY330R cells harbouring pJEG217 had fluorescent foci at the cell membrane, resembling the foci formed by TrhC-GFP. Furthermore, unlike TrhC, these discrete foci were present at both 30 °C and 37 °C, and were found in both the presence and absence of any other drR27 proteins (Fig. 7). When TrhC-GFP was expressed from the expression vector, pMS119EH, foci could not be formed at 30 °C or 37 °C in the absence of drR27 proteins (Gilmour et al., 2001
).
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DISCUSSION |
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In our characterization of the transfer regions of the IncHI1 plasmid R27 we determined that the coupling protein, TraG, is essential for conjugative transfer (Lawley et al., 2002). In this study, we further characterized the coupling protein encoded on the R27 plasmid. A unique feature of the IncHI family of plasmids is that their conjugative transfer is significantly reduced at 37 °C (Taylor & Levine, 1980
). Electron microscopic analysis of cells harbouring R27 plasmid grown at 37 °C revealed an absence of H-pili on the cell surface (Maher et al., 1993
). As pili are required to bring the donor and recipient cells into close proximity, the lack of pili explains the inhibition of transfer at 37 °C. Transcriptional analysis of the Mpf gene, trhC, indicated that transcription was inhibited at 37 °C, thus explaining the lack of H-pili observed during the electron microscopy studies (Gilmour et al., 2001
). The transcription analysis of traG, and the adjacent traI and orf118 genes, at both 30 °C and 37 °C revealed a decrease in the transcript levels at 37 °C, as compared to the RNA levels present at 30 °C. Whereas traG is encoded in the Tra1 region, trhC is encoded within the Tra2 region of R27. The decreased transcript levels of an operon in Tra1 encoding non-Mpf proteins would indicate that a global temperature regulator is controlling R27 conjugation genes in the Tra1 and Tra2 region. A recent analysis of the effect of temperature on R27 transcription has revealed that H-NS and HhaA proteins have an inhibitory effect on the transcription of a number of Tra1 and Tra2 genes at 33 °C (Forns et al., 2005
). A comprehensive analysis of the temperature regulation of each R27 transfer gene has been recently completed (Alonso et al., 2005
).
The C-termini of the coupling family, including the Walker-type NTP-binding domains, show weak similarity with the DNA translocases FtsK and SpoIIIE from E. coli and Bacillus anthracis, respectively (Errington et al., 2001). The SpoIIIE protein has DNA-dependent ATP hydrolysis activity that is used to pump DNA during sporulation (Bath et al., 2000
). The R388 coupling protein also has DNA-dependent ATP hydrolysis activity, and the Walker motifs of R388, RP4 and F plasmid have been demonstrated to be involved in conjugation (Moncalian et al., 1999
; Schroder et al., 2002
; Tato et al., 2005
). Mutational analyses of the Walker A and B motifs of the RP4 coupling protein, TraG, revealed that only two mutations completely abolished RP4 transfer: K187T in Walker A, and D449N in Walker B (Balzer et al., 1994
). NTP-binding studies further determined that the K187T mutation rendered the coupling protein unable to bind ATP (Schroder & Lanka, 2003
). Mutational analysis of the A. tumefaciens coupling protein, VirD4, demonstrated the importance of the Walker A motif (Kumar & Das, 2002
). VirD4 mutants containing the substitutions G151S and K152T were defective in the transfer of both DNA and VirE2 to plant cells. Furthermore, using a transfer DNA immunoprecipitation (TrIP) technique, the VirD4 K152T mutant was found to prevent substrate transfer to the A. tumefaciens T4SS proteins VirB6 and VirB8 (Atmakuri et al., 2004
).
We have expanded the mutational studies of the Walker A and Walker B motifs of the coupling protein family. Substitution of the Gly and Lys residues of the Walker A motif and Asp and Glu residues of the Walker B motifs abolished the capacity of the R27 coupling protein to restore conjugative ability in a complementation assay. A deletion of the Walker A Gly and Lys residues, at positions 210 and 211, had the same effect on the transmission of the R27 plasmid. These results are not unexpected, as alignment of coupling protein homologues indicated that the Gly-Lys and Asp-Glu residues of the Walker A and B motifs, respectively, are found in the majority of coupling proteins (Fig. 2). Notably, the R388 coupling protein TrwB has been identified as a DNA-dependent ATPase (Tato et al., 2005
). The discovery that a coupling protein is able to hydrolyse ATP substantiates the finding that key, well-conserved residues in the Walker A and B regions are necessary for conjugative transfer.
The recent discovery that coupling proteins are able to interact with the VirB10 family of proteins suggests a mechanism by which plasmid DNA moves from the cytoplasm to the membrane-associated T4SS (Gilmour et al., 2003; Llosa et al., 2003
). A more detailed contact pathway has been proposed by tracking the movement of plasmid DNA in A. tumefaciens using the TrIP technique; the T-DNA transfer intermediate interacts with the coupling protein VirD4 initially, and subsequently contacts VirB11, VirB4, VirB6,VirB8, VirB2 and VirB9 (Cascales & Christie, 2004b
). Using non-polar virB mutations, the pathway of the T-DNA substrate has been expanded to propose that VirB10 interacts with the T-DNA after the substrate's interaction with VirB6 and VirB8 (Cascales & Christie, 2004b
). The R27 Mpf protein TrhB, a VirB10 homologue, is probably bitopic, with the majority of the protein extending into the periplasm. TrhB has only 11 residues preceding the single transmembrane domain, as predicted by computational analysis with TMHMM. A 220 aa N-terminal peptide of TrhB (452 aa) retained the ability to interact with the R27 coupling protein TrhB (Gilmour et al., 2003
). Interestingly, a shorter N-terminal peptide of TrhB, 133 aa in length, was not able to bind TraG but was able to interact with full-length TrhB. TrhB contains a proline-rich (17·9 %) region between amino acids 135 and 173; such a proline-rich region is a common feature of VirB10 homologues (Gilmour et al., 2003
). We had postulated that the proline-rich region of TrhB may be involved in the interaction with the coupling protein, TraG (Gilmour et al., 2003
). Within the R27 coupling protein, there are only four residues, Phe-Arg-Ser-Asp, that are predicted to be associated with the periplasm. The BTH screen revealed that a substitution of these residues with four Ser residues was sufficient to abolish a TrhBTraG interaction. The essential role of periplasmic-associated residues in the interaction with TrhB was verified using a co-immunoprecipitation experiment in which an epitope-tagged TrhB was capable of precipitating only WT TraG and not a TraG : S4 construct. Surprisingly, when this coupling protein containing the periplasmic substitutions, TraG : S4, was supplied in trans in a complementation assay with an R27 traG mutant, the TraG : S4 construct was able to restore conjugative ability. The complementation level, however, was almost 1 log lower than the transfer levels of an R27 traG mutant complemented with WT TraG. The ability of the TraG : S4 construct to complement a traG mutation could be explained by the coupling protein interacting with multiple points in the T4SS apparatus, and not solely with TrhB. The BTH and co-immunoprecipitation techniques identify only binary interactions, which is considerably different from the interactions that may occur with the coupling protein and a full complement of R27 T4SS proteins.
The Phe-Arg-Ser-Asp residues of TraG do not represent a common motif within the periplasmic regions of the coupling proteins from the RP4, R388 and F plasmids (Fig. 4). Furthermore, there is significant variability in the number of residues separating the hallmark transmembrane regions of the coupling protein; TraD had the largest number of periplasmic-associated residues, with 62 aa, and TraG of R27 had the smallest number, with only 4 aa separating the transmembrane regions. One common feature of the coupling protein family is the interchangeability of the coupling proteins between non-cognate T4SS (Cabezon et al., 1994
; Hamilton et al., 2000
). This has been further demonstrated using BTH technology in which the R388 VirB10 homologue, TrwE, was found to interact with non-cognate coupling proteins from the IncN plasmid pKM101 and IncX plasmid R6K (Llosa et al., 2003
). The R27 VirB10 homologue, TrhB, has also been found to interact with non-cognate coupling proteins encoded on the F, RP4 and R388 plasmids (J. Gunton & D. E. Taylor, unpublished). The BTH and immunoprecipitation data obtained with the R27 TraG : S4 construct suggest that the periplasmic region is essential for the interaction with TrhB. A shared feature of the VirB10 homologues is the proline-rich region in the N-terminus. This structural feature may be interacting in a non-specific fashion, with the periplasmic residues of the coupling protein, thus allowing for the observed interchangeability of coupling proteins between heterologous T4SS.
Immunofluorescence microscopy was used to determine that R27 TraGHis6 protein forms multiple fluorescent foci within the periphery of the cell. Similar foci were observed when GFP was fused to the C-terminus of the R27 Mpf protein, TrhC (Gilmour et al., 2001). Notably, DY330R cells containing TraGHis6 or TrhC-GFP formed the same number of foci in the cellular membrane; there was an average of five to six foci in cells containing the R27 coupling protein or TrhC. With both TraG and TrhC, foci were found throughout the cell periphery, with a moderate bias towards the quarter and polar positions of the cell (Gilmour et al., 2001
). The position of R27 protein-dependent foci in the cell is strikingly different from the position of the R27 plasmid DNA; GFP-labelled R27 plasmid DNA localized to discrete positions at the mid and quarter cell position (Gilmour et al., 2001
; Lawley & Taylor, 2003
). Electron microscopy revealed that the H-pilus, product of the R27 T4SS, can assemble and extend from random positions on the cell membrane and is not limited to this mid or quarter cell position (Gilmour et al., 2001
).
As R27 conjugation is influenced by temperature, TraG-dependent formation of fluorescent foci was investigated in cells grown at 37 °C. Although foci were found at both 30 °C and 37 °C there was a statistically significant decrease in the number of foci formed when cells expressing TraG alone were grown at 37 °C instead of at 30 °C, a temperature that is permissive for R27 conjugative transfer (P=0·001). Furthermore, there was a significant change in the number of foci at 30 °C when cells expressing TraG also harboured the R27 plasmid (P=0·028). These data suggest that in the absence of essential R27 proteins, the number of TraG-associated foci per cell is slightly higher at 30 °C, as compared to the number of foci formed at 37 °C; temperature may be involved in more than simply transcriptional control of the R27 genome. Additionally, in the presence of R27 proteins, the number of TraG foci decreases when compared to cells expressing TraG alone. As expected, this decrease is not significantly different in the presence and absence of pDT3152 at 37 °C, as at this elevated temperature, transcription of the majority of R27 genes is significantly reduced (Gilmour et al., 2001; Alonso et al., 2005
).
The ability of a coupling protein to localize to discrete positions within the cell, in the absence of other T4SS proteins, is not a unique phenomenon. The A. tumefaciens coupling protein, VirD4, localized to the poles of the cell, independent of other Vir proteins or a T4SS apparatus (Kumar & Das, 2002). The A. tumefaciens T4SS protein VirB6 also localizes to the poles; however, like TrhC from the R27 plasmid, this localization is dependent on the presence of a subset of conjugative proteins, VirB7VirB11 (Judd et al., 2005
). However, this dependence of VirB6 positioning on Ti-plasmid-encoded VirB proteins was not demonstrated in a recent study, suggesting that additional work is required to resolve the architecture and temporal assembly of the Vir T4SS (Jakubowski et al., 2004
).
In conclusion, the TraG periplasmic-spanning residues and well-conserved residues in the Walker-type ATP-binding domains have been shown to be involved in the functionality of the R27 coupling protein. Moreover, the independent cellular localization of foci formed by the coupling protein is similar in position and number to that seen for potential T4SS complexes encoded by the R27 plasmid. These data support a model of conjugation in which the coupling protein localizes to the periphery of the cell and associates with the T4SS protein TrhB with periplasmic-spanning residues, thus enabling plasmid DNA to traverse the donor cell envelope.
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ACKNOWLEDGEMENTS |
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Received 9 June 2005;
revised 19 August 2005;
accepted 22 August 2005.
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