| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
1,2
1 Department for Environmental Microbiology, University of Technology Berlin, FR1-2, Franklinstrasse 28/29, D-10587 Berlin, Germany
2 Institute for Chemistry, Karl-Franzens-Universität Graz, Heinrichstrasse 28, A-8010 Graz, Austria
Correspondence
Elisabeth Grohmann
elisabeth.grohmann{at}tu-berlin.de
 |
ABSTRACT |
|---|
 TOP ABSTRACT INTRODUCTIONMETHODSRESULTS AND DISCUSSIONREFERENCES |
|---|
-Galactosidase assays with Ptra–lacZ fusions proved Ptra promoter activity, which was strongly repressed when TraA was supplied in trans. Thus, it is concluded that the pIP501 tra operon is negatively autoregulated at the transcriptional level by the conjugative DNA relaxase TraA.
Present address: Competence Center for Fluorescence Analysis, Josef-Engert-Strasse 9, D-93053 Regensburg, Germany.
|
INTRODUCTION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTS AND DISCUSSIONREFERENCES |
|---|
), conferring resistance to the MLS group of antibiotics (erythromycin) and to chloramphenicol. pIP501 exhibits a very broad host range for conjugative transfer, including streptococci, lactobacilli, enterococci, lactococci, staphylococci, bacilli, Listeria and clostridia. Recently, Zuniga and co-workers have transferred pIP501 and derivatives thereof to Oenococcus oeni, a lactic acid bacterium used as a commercial starter culture, and for which no suitable genetic tools for transfer of exogenous DNA are available (Zuniga et al., 2003). We have demonstrated conjugative transfer of pIP501 to the multicellular Gram-positive (G+) organism Streptomyces lividans and to the Gram-negative (G–) organism Escherichia coli. The pIP501 antibiotic resistance, replication and tra genes are functional in the heterologous hosts, and the plasmid is stably maintained for at least 50 generations in E. coli XL-1 Blue cells (Kurenbach et al., 2003).
The pIP501 nic site, at which plasmid DNA transfer initiates by the relaxase-mediated introduction of a site- and strand-specific nick, has been mapped by Wang & Macrina (1995a). They also proved in vivo nicking activity of the first gene product encoded by the operon, the TraA relaxase (Wang & Macrina, 1995b). TraA- and TraAN293- (the protein comprising the N-terminal 293 amino acids of TraA) mediated in vitro relaxation of supercoiled oriTpIP501 DNA has been demonstrated by Kurenbach et al. (2002), and relaxation activity of TraAN246 (the protein comprising the N-terminal 246 amino acids of TraA) by Kope et al. (2005). The pIP501 relaxase TraA contains a positively charged tail sequence at the C terminus, as found in putative type IV secretion substrates and in relaxases of conjugative plasmids from various 
-Proteobacteria (Schulein et al., 2005). Ptra has been mapped by primer extension analysis. Co-transcription of the tra genes, orf1 to orf11, has been shown by RT-PCR on RNA from Enterococcus faecalis cells harbouring pIP501 (Kurenbach et al., 2002).
Three of the pIP501 tra genes exhibit significant similarity to type IV secretion system components (Grohmann et al., 2003; Kurenbach et al., 2003) involved in conjugative transfer in G– bacteria (for a review see Llosa & de la Cruz, 2005) and transport of effector molecules from G– pathogens to eukaryotic host cells (reviewed by Cascales & Christie, 2003; Christie, 2004; Christie et al., 2005; Christie & Cascales, 2005). Possible roles for the type IV homologues in a presumably simplified type IV secretion process through the G+ cell envelope have been discussed in Grohmann et al. (2003) and Grohmann (2005).
Regulation of conjugative transfer has been studied in some detail for G– bacteria, whereas in G+ bacteria knowledge of regulation of conjugative transfer is mainly based on data of the Ent. faecalis sex-pheromone-responding conjugative plasmids pCF10, pAD1 and pPD1 (Bae & Dunny, 2001; Bae et al., 2002, 2004; Horii et al., 2002; for reviews see Clewell & Dunny, 2002; Chandler & Dunny, 2004).
In this report, we present data on the regulation of the pIP501 tra operon (Fig. 1). By two different approaches we demonstrate that the regulation is exerted at the transcriptional level: i) Ptra : : lacZ reporter fusions proved repression of the tra operon promoter in the presence of the TraA DNA relaxase; and ii) electrophoretic mobility shift assays (EMSAs) and DNase I protection experiments showed binding of TraA to DNA fragments containing the tra operon promoter and parts thereof.
|
|
METHODS |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTS AND DISCUSSIONREFERENCES |
|---|
) was cultivated in brain heart infusion medium (Oxoid) at 37 °C. For the selection of Ent. faecalis JH2-2 (pIP501), 20 µg chloramphenicol ml–1 was added to the medium. E. coli JM109 (Promega) and E. coli HB101 (Promega) were grown in LB medium at 37 °C, supplemented with 100 µg ampicillin ml–1 for the selection of pQE30-traAN246 (Kope et al., 2005) and pQF120 (Ronald et al., 1990) and derivatives thereof. LB medium was supplemented with 20 µg chloramphenicol ml–1 and 10 µg tetracycline ml–1 for the selection of pACYC184, and supplemented with 20 µg chloramphenicol ml–1 alone for derivatives thereof. For the -galactosidase assays, E. coli JM109 cells harbouring the respective plasmids were cultivated in the medium suggested by Miller (1972).
DNA preparation and transformation.
Extraction and purification of plasmid DNAs from E. coli were performed using the Qiagen kit or the Gen Elute Plasmid Miniprep kit (Sigma). Restriction endonucleases were purchased from Promega and New England Biolabs, T4 DNA ligase and Shrimp alkaline phosphatase from Roche Diagnostics, and Gen Therm DNA polymerase from Rapidozym. The enzymes were used as specified by the suppliers. PCR fragments for cloning experiments were purified by Wizard PCR Preps (Promega). Preparation of competent cells and E. coli transformations with plasmid DNA were performed by standard methods (Sambrook et al., 1989).
Construction of plasmids for the -galactosidase assay.
The promoter probe plasmid pQF120 containing a promoterless lacZ gene was used to clone Ptra. Ptra was amplified as a 179 bp PCR fragment with the oligonucleotide primers Ptra_fw and Ptra_rev with added BglII restriction sites at their 5' ends and a lysate of Ent. faecalis JH2-2 (pIP501) as template. All oligonucleotides used in this work are listed in Table 1. The 171 bp BglII–BglII fragment was ligated with BglII-cut and dephosphorylated pQF120 (9200 bp). E. coli JM109 cells harbouring recombinant plasmids (pQF120-Ptra) were selected as blue colonies on LB agar plates supplemented with 100 µg ampicillin ml–1 and 40 µg X-Gal ml–1. Ptac and the glutathione S-transferase gene (Ptac : : GST) were PCR-amplified from pGEX-2T (Amersham Biosciences) with primers containing SalI and SphI restriction sites at the 5' ends, respectively; the fragment was cut with SalI/SphI and inserted into the respective sites of pACYC184 (Chang & Cohen, 1978), thereby interrupting the tetracycline-resistance gene. The traA expression cassette (Ptac : : GST-traA) was amplified from pGEX-2T-traA (Kurenbach et al., 2002) with the same primers and inserted into the SalI/SphI sites of pACYC184. Transformants resistant to chloramphenicol but sensitive to tetracycline were PCR-verified for the presence of Ptac : : GST and Ptac : : GST-traA, respectively. The nucleotide sequence of the insertions was verified by dideoxy chain termination sequencing in an automated sequencer (ABI prism 310, Perkin Elmer).
|
-Galactosidase assay.-galactosidase activity was performed as described by Miller (1972).
Estimation of plasmid copy number.
Aliquots taken from cultures at the time of sampling for -galactosidase assays were lysed, and plasmid DNA was prepared with the Gen Elute Plasmid Miniprep kit (Sigma) and analysed on 0·7 % agarose gels. The gels were stained and the amount of plasmid DNA per unit of culture optical density quantified by the Easy win 32 software (Herolab).
RT-PCR analysis.
RNA of exponentially growing Ent. faecalis JH2-2 and Ent. faecalis JH2-2 cells harbouring pIP501 (OD600=0·6) was isolated and purified as described in Kurenbach et al. (2002). RT-PCR was performed with primer pairs designed to amplify two successive ORFs (orf11 to orf15) in the pIP501 tra region. Prior to use in RT-PCR, RNA was treated with DNase I (Promega). A 0·5 µg quantity of RNA and 50 pmol of each primer were used in each RT-PCR performed with the Access-RT-PCR kit (Promega). RNA samples were denatured for 2 min at 70 °C and kept on ice prior to addition of polymerases. The orf11 to orf12 fragment was amplified as follows: 48 °C for 60 min for reverse transcription, followed by inactivation of avian myeloblastosis virus reverse transcriptase (AMV-RT) and denaturation of the template at 94 °C for 90 s. The program 94 °C for 30 s/55 °C for 90 s/68 °C for 4 min was applied (40 cycles) and terminated by a final elongation step of 10 min. For the amplification of orf12 to orf13, orf13 to orf14, orf14 to orf15, and orf15 to copR, the program 94 °C for 30 s/60 °C for 90 s/68 °C for 2 min (30 cycles) was applied and terminated by a final elongation step of 10 min. Control reactions were performed with RNA from the plasmid-free isogenic strain, without template RNA, and with template RNA but omitting the reverse transcription step (data not shown). RT-PCR products were analysed on 2 % agarose gels.
RT-PCR of tra mRNA isolated under different growth conditions.
Total RNA was isolated from Ent. faecalis JH2-2 (pIP501) cells harvested at different stages of bacterial growth: in the early exponential phase, OD600=0·2; in the mid-exponential phase, OD600=0·6; and during the stationary growth phase, OD600=1·0. The semi-quantitative RT-PCR was performed in two steps. i) Reverse transcription (cDNA synthesis): 2 µl DNase-treated RNA was incubated with 0·5 µg random hexamer primer (Promega) in a volume of 5 µl for 5 min at 70 °C, and then stored on ice. dNTPs (10 pmol), 2 mM MgCl2, 4 µl 5x M-MLV buffer and 1 µl M-MLV (Moloney murine leukaemia virus) reverse transcriptase and diethyl pyrocarbonate-treated water were added to a final volume of 20 µl and incubated for 5 min at 25 °C, 60 min at 42 °C and 15 min at 70 °C; cDNA was purified by ethanol precipitation. The DNA concentration was determined by A260 measurement and calculated by using the online help (www.promega.com/biomath) for single-strand DNA calculations. ii) PCR: 1 µg cDNA was applied to PCRs containing 2 mM MgCl2, 10 pmol dNTPs, 5 µl 10x PCR buffer, 1·5 U Gentherm DNA polymerase and 20 pmol of each primer in a total volume of 50 µl. For amplification of orf1 to orf2, orf6 to orf7, and orf13 to orf14, the cycle program 94 °C for 30 s/60 °C for 90 s/68 °C for 2 min (30 cycles) was applied and terminated by a final elongation step of 10 min. As a constitutively expressed control, the glyceraldehyde-3-phosphate dehydrogenase (GAP-DH) gene was reverse transcribed and amplified by the same procedure. For amplification of orf3 to orf4 and the gene encoding GAP-DH, the annealing temperature was decreased to 56 °C. The PCR products were analysed in 1·5 % agarose gels and quantified by the Easy win 32 software (Herolab).
DNA labelling.
Synthetic oligonucleotides were purchased from VBC-GENOMICS and Sigma-Genosys. They were labelled with [
32P]ATP (1·11x1014 Bq mmol–1) by T4 polynucleotide kinase (Roche Diagnostics). Unbound [32P]ATP was removed by a Sephadex G-50 (Amersham Biosciences) column. For EMSAs, the 5' end-labelled oligonucleotides were annealed to the complementary unlabelled oligonucleotide to generate double-stranded DNA. A 1 : 1 mixture of the oligonucleotides was diluted in Tris/EDTA buffer (10 : 1), completely denatured (5 min at 95 °C) and annealed by slowly cooling down to room temperature. The labelled DNA fragments were applied immediately to the EMSAs or stored at 4 °C.
EMSAs.
TraAN246 was overexpressed and purified as described in Kope et al. (2005). All oligonucleotides used to generate double-stranded DNA fragments are shown in Table 1
. Binding mixtures (20 µl) containing 10 fmol radiolabelled DNA fragment and increasing TraAN246 concentrations in 20 mM Tris/HCl, pH 7·5, 0·1 mM EDTA, 200 mM NaCl, were incubated at 37 °C. Binding reactions and electrophoresis were performed as described in Kope et al. (2005). As a negative control, a randomly chosen 42-mer DNA fragment with no sequence identity with the pIP501 promoter region (nucleotides 2179 to 2220 on pIP501, accession no. AJ301605) was incubated with increasing TraAN246 concentrations up to 4 µM. No binding was observed.
DNase I footprint.
5'-Labelled FP_forward and unlabelled FP_reverse primer or 5'-labelled FP_reverse and unlabelled FP_forward primer were used to generate a 250 bp Ptra and oriT DNA fragment (nucleotides 1097 to 1346, accession no. L39769) with labelled coding and non-coding strands.
Prior to the DNase I footprint reaction, the fragments were heated to 95 °C for 10 min and allowed to cool to 37 °C. TraA was purified as described in Kope et al. (2005). Ten nanograms of the 250 bp fragment (6·5 nM) were incubated at 37 °C for 10 min with increasing TraA concentrations from 200 nM to 2 µM in binding buffer (20 mM Tris/HCl, pH 8·0, 200 mM NaCl, 0·1 mM EDTA) in a total volume of 10 µl. DNase I (0·01 Kunitz units, Fermentas) was added to each sample. Ten microlitres of stop buffer (100 µg yeast tRNA ml–1, 30 mM EDTA, 1 % SDS, 200 mM NaCl) (Leblanc & Moss, 1994) were added to naked DNA after 1 min, and to reactions with TraA after 3 min. DNA was extracted with phenol/chloroform/isoamyl alcohol (25 : 24 : 1, by volume) and precipitated with ethanol. The pellets were air-dried, dissolved in loading buffer (33 mM NaOH, 32 % formamide, 0·1 % bromophenol blue, 0·1 % xylene cyanol) and run on a 5 % denaturing polyacrylamide gel with 8 M urea in 1x TBE buffer at constant wattage. Reference sequencing reactions were prepared with the Cycle Sequencing kit (Fermentas) with primers FP_forward and FP_reverse. Only the nucleotide numbers are shown in Fig. 5. The gel was exposed overnight to a Storage Phosphor GP Screen (Amersham Biosciences) and read by the Typhoon 9400 imaging system (Amersham Biosciences).
|
|
RESULTS AND DISCUSSION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTS AND DISCUSSIONREFERENCES |
|---|
). RT-PCR resulted in products of the expected size for orf11 to orf12, orf12 to orf13, orf13 to orf14, and orf14 to orf15 (Fig. 2, lanes 1, 2, 3 and 4). We tested for the existence of transcription products beyond orf15 using primers which would generate an orf15/copR product of 480 bp. Using RNA as template, the respective product was never observed (Fig. 2, lane 5). Transcription of the pIP501 tra operon appears to be terminated by a strong rho-independent transcriptional terminator [free energy of about –46 kJ mol–1, for the following setting: DNA sequence at 37 °C, 1 M NaCl; MFold web server for nucleic acid folding and hybridization prediction: http://www.bioinfo.rpi.edu/applications/mfold (Zuker, 2003)] approximately 10 bp downstream of the orf15 translational stop codon (data not shown).
|
, PCR samples of orf1 to orf2, orf13 to orf14, and GAP-DH are shown. The amounts of obtained PCR products were compared for the different tra gene fusions at the three different time-points by quantification of the DNA bands with Easy win 32 software. No significant differences were detected for the analysed PCR products. The constitutively expressed gene for GAP-DH yielded the same amount of PCR product under all the conditions tested.
|
), was never observed. The expression of several F-encoded tra genes decreases at the transcriptional level in mid-exponential or stationary phase, coincident with a rapid decline in transfer efficiency in mid-exponential phase (Frost & Manchak, 1998). We conclude that the pIP501 tra genes are expressed during the whole growth cycle of Ent. faecalis and that their level of expression is independent of growth phase.
The TraA relaxase binds to the Ptra promoter
The compact organization of the pIP501 oriT region (Fig. 4), in the sense that the Ptra –10 and –35 boxes overlap with the left half repeat of inverted repeat structures (IR-1 and IR-2), presumably representing the TraA recognition and binding site (Kope et al., 2005), makes autoregulation of the tra operon by the TraA relaxase likely. To study relaxase binding to the Ptra promoter, we selected three DNA fragments, the first comprising the whole promoter (–35 and –10 region), the second the –35 region alone, and the third the –10 region alone. The shortest N-terminal portion of TraA exhibiting relaxase activity, the 246 amino acid TraAN246 protein (Kope et al., 2005), was used in the bandshift assays. The oligonucleotide representing the tra coding strand was 5' labelled and annealed to the complementary unlabelled strand to generate double-stranded substrates for the EMSAs. As an example, the data for the –10 region fragment are shown. Applying increasing TraAN246 concentrations to this fragment, we detected one retarded DNA–protein complex (Fig. 4).
|
The complete left half repeat of IR-2 was present in all single-strand oligonucleotides shown to bind TraAN246 and TraA. An oligonucleotide comparable with the –10 region fragment, but additionally containing the right half repeat, results in similar binding affinity (Kope et al., 2005). TraA showed similar binding affinities for the different promoter fragments to those of the N-terminal domain TraAN246 (data not shown).
Incubation of TraAN246 at concentrations up to 4 µM with a 42-mer control fragment (8000-fold excess of protein) resulted in no visible shift (data not shown). We conclude that the TraA DNA relaxase binds to the Ptra promoter region. This is in good agreement with relaxase binding to oligonucleotides composed of i) the complete IR-2 structure, ii) IR-2 and the region up to the nic site, and iii) IR-2, the nic site and seven further 5' bases (Kope et al., 2005).
DNase I footprinting analyses with a 250 bp DNA fragment composed of Ptra and the complete IR-1 and IR-2 structures showed protection of both the Ptra –35 region and the –10 region, with hypersensitive sites on the non-cleaved strand close to the nic site (nucleotide numbers 1253 and 1256), at the nic site (nucleotide number 1262) and two nucleotides downstream from the –10 region. On the cleaved strand, DNase I protection extends eight nucleotides to the nic site, with the nic site itself as hypersensitive site (Fig. 5). The DNase I hypersensitive sites could be generated by a conformational change of the oriT region induced by TraA binding, resulting in greater exposure to DNase I attack.
Our data indicate that the left half repeats of IR-1 and IR-2 are the preferential binding sites for the TraA relaxase. Binding of TraA to its target DNA would be a prerequisite for the recognition and cleavage of DNA at the 5'-GpC-3' dinucleotide in the nic site, which would remain accessible to the enzymic activity of TraA.
Autoregulation of the tra operon: the TraA relaxase negatively regulates transcription from the Ptra promoter
To prove that TraA binding to the Ptra promoter region affects promoter activity, we put the promoterless lacZ gene in pQF120 under the control of the Ptra promoter. E. coli JM109 cells harbouring this construct, pQF120-Ptra : : lacZ, gave blue colonies on LB X-Gal plates and resulted in a -galactosidase activity of 401 Miller units. The effect of traA expression in trans on Ptra activity was tested by co-transformation of E. coli JM109 cells with pQF120-Ptra : : lacZ and pACYC184-Ptac : : GST-traA expressing traA under the control of the IPTG-inducible tac promoter. When traA expression was induced by the addition of 1 mM IPTG, the -galactosidase activity dropped to 6 Miller units. As a control, the effect of co-resident pACYC184-Ptac : : GST on the Ptra activity of pQF120-Ptra : : lacZ was tested. No significant change in -galactosidase activity (407 Miller units) was observed. The copy number of the pACYC184 derivatives (pACYC184-Ptac : : GST and pACYC184-Ptac : : GST-traA) is considerably smaller (10–12 copies per cell) than that of pQF120-Ptra : : lacZ (500–700 copies per cell, pMB1 ori of pUC18). The -galactosidase activities were corrected for apparent copy-number variations. The data (mean values of three independent measurements) clearly indicate that the tra operon is regulated at the level of transcription by the TraA relaxase.
The compact organization of the pIP501 oriT region: partial overlapping of relaxase promoter and nic-region, resembles that of the rolling-circle-replicating plasmid pMV158 (Farías et al., 1999; Grohmann et al., 1999), which is efficiently mobilized by pIP501 (van der Lelie et al., 1990; Kurenbach et al., 2003). For the pMV158-encoded relaxase MobM, autoregulation is currently under investigation. de Antonio and co-workers have proposed that a Leu-zipper motif between residues 317 and 338 in MobM might be involved in dimerization and autoregulation (de Antonio et al., 2004). In TraA, no putative Leu-zipper motif was found. For Mob, the mobilization protein encoded by the mobilizable broad-host-range plasmid pBBR1, the nic site of which is identical with that of pMV158, autoregulation by the binding of Mob to its promoter region overlapping with oriT has been demonstrated (Szpirer et al., 2001).
Autoregulation of tra gene expression mediated by the transfer initiator protein, the DNA relaxase, seems to be an effective mechanism to shut down the energy-consuming process of plasmid transfer in a controlled way at a very early stage of plasmid spread. It has been demonstrated that this mechanism is not restricted to small non-self-transmissible plasmids, but seems also to control the conjugative transfer of multiple resistance plasmids of G+ origin (pIP501 and pRE25, the transfer region of which is virtually identical to that of pIP501). All these transfer-control systems as well as those from G– bacteria appear to be designed to achieve an optimum balance between the maximum transfer potential and the lowest metabolic burden for the host.
|
ACKNOWLEDGEMENTS |
|---|
|
REFERENCES |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTS AND DISCUSSIONREFERENCES |
|---|
Bae, T., Kozlowicz, B. K. & Dunny, G. M. (2002). Two targets in pCF10 DNA for PrgX binding: their role in production of Qa and prgX mRNA and in regulation of pheromone-inducible conjugation. J Mol Biol 315, 995–1007.[CrossRef][Medline]
Bae, T., Kozlowicz, B. K. & Dunny, G. M. (2004). Characterization of cis-acting prgQ mutants: evidence for two distinct repression mechanisms by Qa RNA and PrgX protein in pheromone-inducible enterococcal plasmid pCF10. Mol Microbiol 51, 271–281.[CrossRef][Medline]
Cascales, E. & Christie, P. J. (2003). The versatile bacterial type IV secretion systems. Nat Rev Microbiol 1, 137–149.[CrossRef][Medline]
Chandler, J. R. & Dunny, G. M. (2004). Enterococcal peptide sex pheromones: synthesis and control of biological activity. Peptides 25, 1377–1388.[CrossRef][Medline]
Chang, A. C. Y. & Cohen, S. N. (1978). Construction and characterization of amplifiable multicopy DNA cloning vehicles derived from the P15A cryptic miniplasmid. J Bacteriol 134, 1141–1156.
Christie, P. J. (2004). Type IV secretion: the Agrobacterium VirB/D4 and related conjugation systems. Biochim Biophys Acta 1694, 219–234.[Medline]
Christie, P. J. & Cascales, E. (2005). Structural and dynamic properties of bacterial type IV secretion systems. Mol Membr Biol 22, 51–61.[Medline]
Christie, P. J., Atmakuri, K., Krishnamoorthy, V., Jakubowski, S. & Cascales, E. (2005). Biogenesis, architecture, and function of bacterial type IV secretion systems. Annu Rev Microbiol (in press).
Clewell, D. B. & Dunny, G. M. (2002). Conjugation and genetic exchange in Enterococci. In The Enterococci: Pathogenesis, Molecular Biology, and Antibiotic Resistance, 1st edn, pp. 265–300. Edited by M. S. Gilmore, D. B. Clewell, P. Courvalin, G. M. Dunny, B. E. Murray & L. B. Rice. Washington, DC: American Society for Microbiology.
de Antonio, C., Farías, M. E., de Lacoba, M. G. & Espinosa, M. (2004). Features of the plasmid pMV158-encoded MobM, a protein involved in its mobilization. J Mol Biol 335, 733–743.[CrossRef][Medline]
Farías, M. E., Grohmann, E. & Espinosa, M. (1999). Expression of the mobM gene of the streptococcal plasmid pMV158 in Lactococcus lactis subsp. lactis. FEMS Microbiol Lett 176, 403–410.[Medline]
Frost, L. S. & Manchak, J. (1998). F– phenocopies: characterization of expression of the F transfer region in stationary phase. Microbiology 144, 2579–2587.[Abstract]
Grohmann, E. (2005). Cell–cell channels in conjugating bacteria. In Cell–Cell Channels. Edited by F. Baluska, D. Volkmann & P. W. Barlow. Georgetown, TX: Landes Bioscience (in press).
Grohmann, E., Guzmán, L. M. & Espinosa, M. (1999). Mobilisation of the streptococcal plasmid pMV158: interactions of MobM protein with its cognate oriT DNA region. Mol Gen Genet 261, 707–715.[CrossRef][Medline]
Grohmann, E., Muth, G. & Espinosa, M. (2003). Conjugative plasmid transfer in Gram-positive bacteria. Microbiol Mol Biol Rev 67, 277–301.
Hayes, W. (1964). The Genetics of Bacteria and their Viruses. New York: Wiley.
Horii, T., Nagasawa, H. & Nakayama, J. (2002). Functional analysis of TraA, the sex pheromone receptor encoded by pPD1, in a promoter region essential for the mating response in Enterococcus faecalis. J Bacteriol 184, 6343–6350.
Horodniceanu, T., Bouanchaud, D. H., Bieth, G. & Chabbert, Y. A. (1976). R plasmids in Streptococcus agalactiae (group B). Antimicrob Agents Chemother 10, 795–801.
Jacob, A. E. & Hobbs, S. J. (1974). Conjugal transfer of plasmid-borne multiple antibiotic resistance in Streptococcus faecalis var. zymogenes. J Bacteriol 117, 360–372.
Kope, J., Bergmann, A., Fritz, G., Grohmann, E. & Keller, W. (2005). TraA and its N-terminal relaxase domain of the Gram-positive plasmid pIP501 show specific oriT binding and behave as dimers in solution. Biochem J 387, 401–409.[CrossRef][Medline]
Kurenbach, B., Grothe, D., Farías, M. E., Szewzyk, U. & Grohmann, E. (2002). The tra region of the conjugative plasmid pIP501 is organized in an operon with the first gene encoding the relaxase. J Bacteriol 184, 1801–1805.
Kurenbach, B., Bohn, C., Prabhu, J., Abudukerim, M., Szewzyk, U. & Grohmann, E. (2003). Intergeneric transfer of the Enterococcus faecalis plasmid pIP501 to Escherichia coli and Streptomyces lividans and sequence analysis of its tra region. Plasmid 50, 86–93.[CrossRef][Medline]
Leblanc, B. & Moss, T. (1994). Dnase I footprinting. In DNA–Protein Interactions, Principles and Protocols (Methods in Molecular Biology vol. 30), pp. 1–10. Edited by G. G. Kneale. Tatowa, NJ: Humana Press.
Llosa, M. & de la Cruz, F. (2005). Bacterial conjugation: a potential tool for genomic engineering. Res Microbiol 156, 1–6.[Medline]
Miller, J. H. (1972). Experiments in Molecular Genetics, 1st edn. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory.
Ronald, S. L., Kropinski, A. M. & Farinha, M. A. (1990). Construction of broad-host-range vectors for the selection of divergent promoters. Gene 90, 145–148.[CrossRef][Medline]
Sambrook, J., Fritsch, E. F. & Maniatis, T. (1989). Molecular Cloning: a Laboratory Manual, 2nd edn. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory.
Schulein, R., Guye, P., Rhomberg, T. A., Schmid, M. C., Schroder, G., Vergunst, A. C., Carena, I. & Dehio, C. (2005). A bipartite signal mediates the transfer of type IV secretion substrates of Bartonella henselae into human cells. Proc Natl Acad Sci U S A 102, 856–861.
Szpirer, C. Y., Faelen, M. & Couturier, M. (2001). Mobilization function of the pBHR1 plasmid, a derivative of the broad-host-range plasmid pBBR1. J Bacteriol 183, 2101–2110.
van der Lelie, D., Wösten, H. A., Bron, S., Oskam, L. & Venema, G. (1990). Conjugal mobilization of streptococcal plasmid pMV158 between strains of Lactococcus lactis subsp. lactis. J Bacteriol 172, 47–52.
Wang, A. & Macrina, F. L. (1995a). Streptococcal plasmid pIP501 has a functional oriT site. J Bacteriol 177, 4199–4206.
Wang, A. & Macrina, F. L. (1995b). Characterization of six linked open reading frames necessary for pIP501-mediated conjugation. Plasmid 34, 206–210.[CrossRef][Medline]
Zuker, M. (2003). MFold web server for nucleic acid folding and hybridization prediction. Nucleic Acids Res 31, 3406–3415.
Zuniga, M., Pardo, I. & Ferrer, S. (2003). Conjugative plasmid pIP501 undergoes specific deletions after transfer from Lactococcus lactis to Oenococcus oeni. Arch Microbiol 180, 367–373.[CrossRef][Medline]
Received 25 August 2005;
revised 15 November 2005;
accepted 17 November 2005.
This article has been cited by other articles:
|
|
 |
|
  Y. Chen, X. Zhang, D. Manias, H.-J. Yeo, G. M. Dunny, and P. J. Christie Enterococcus faecalis PcfC, a Spatially Localized Substrate Receptor for Type IV Secretion of the pCF10 Transfer Intermediate J. Bacteriol., May 15, 2008; 190(10): 3632 - 3645. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
M. Y. Abajy, J. Kopec, K. Schiwon, M. Burzynski, M. Doring, C. Bohn, and E. Grohmann A Type IV-Secretion-Like System Is Required for Conjugative DNA Transport of Broad-Host-Range Plasmid pIP501 in Gram-Positive Bacteria J. Bacteriol., March 15, 2007; 189(6): 2487 - 2496. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
| INT J SYST EVOL MICROBIOL | MICROBIOLOGY | J GEN VIROL |
| J MED MICROBIOL | ALL SGM JOURNALS | |
