Genome-Scale Analysis of Mycoplasma agalactiae Loci Involved in Interaction with Host Cells

doi:10.1371/journal.pone.0025291

PLoS One. 2011; 6(9): e25291.

Published online 2011 September 23. doi: 10.1371/journal.pone.0025291

PMCID: PMC3179502

Copyright Skapski et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.

Genome-Scale Analysis of Mycoplasma agalactiae Loci Involved in Interaction with Host Cells

Agnès Skapski,^1,² Marie-Claude Hygonenq,^1,² Eveline Sagné,^1,² Sébastien Guiral,^1,²^¤ Christine Citti,^1,² and Eric Baranowski^1,²^*

¹INRA, UMR1225, IHAP, Toulouse, France

²Université de Toulouse, INP, ENVT, UMR1225, IHAP, Toulouse, France

Olivier Neyrolles, Editor

Institut de Pharmacologie et de Biologie Structurale, France

* E-mail: e.baranowski/at/envt.fr

Conceived and designed the experiments: AS CC EB. Performed the experiments: AS M-CH ES SG EB. Analyzed the data: AS CC EB. Contributed reagents/materials/analysis tools: SG. Wrote the paper: AS CC EB.

^¤Current address: Institut de Biologie et Chimie des Protéines,CNRS, Université de Lyon, Lyon, France

Received July 4, 2011; Accepted August 31, 2011.

Abstract

Mycoplasma agalactiae is an important pathogen of small ruminants, in which it causes contagious agalactia. It belongs to a large group of “minimal bacteria” with a small genome and reduced metabolic capacities that are dependent on their host for nutrients. Mycoplasma survival thus relies on intimate contact with host cells, but little is known about the factors involved in these interactions or in the more general infectious process. To address this issue, an assay based on goat epithelial and fibroblastic cells was used to screen a M. agalactiae knockout mutant library. Mutants with reduced growth capacities in cell culture were selected and 62 genomic loci were identified as contributing to this phenotype. As expected for minimal bacteria, “transport and metabolism” was the functional category most commonly implicated in this phenotype, but 50% of the selected mutants were disrupted in coding sequences (CDSs) with unknown functions, with surface lipoproteins being most commonly represented in this category. Since mycoplasmas lack a cell wall, lipoproteins are likely to be important in interactions with the host. A few intergenic regions were also identified that may act as regulatory sequences under co-culture conditions. Interestingly, some mutants mapped to gene clusters that are highly conserved across mycoplasma species but located in different positions. One of these clusters was found in a transcriptionally active region of the M. agalactiae chromosome, downstream of a cryptic promoter. A possible scenario for the evolution of these loci is discussed. Finally, several CDSs identified here are conserved in other important pathogenic mycoplasmas, and some were involved in horizontal gene transfer with phylogenetically distant species. These results provide a basis for further deciphering functions mediating mycoplasma-host interactions.

Introduction

The term “mycoplasma” is used trivially to describe bacteria belonging to the class Mollicutes, which includes the genus Mycoplama, as well as several other related genera [1]. These micro-organisms have evolved from a low G+C content Gram positive ancestor by “regressive evolution”, resulting in massive genome reduction [2], [3]. As a result, contemporary mycoplasmas lack a cell-wall and are commonly described as the smallest self-replicating organisms, because of the small size of their genome (580 to 1,400 kbp) and the paucity of their metabolic pathways. Mycoplasmas and ureaplasmas live in close contact with animal tissues, probably because of their limited metabolic capacity, a feature that is likely to have increased their dependence on hosts for a number of nutrients [2]. Mycoplasmas occur widely in nature and, despite their apparent simplicity, several species are successful pathogens of animals, in which they establish persistent infections and cause chronic disease [4].

Mycoplasma agalactiae is an important pathogen of small ruminants that causes contagious agalactia (CA), resulting in significant losses in the sheep and goat milk industries [5]. It is classified by the World Organization for Animal Health (OIE) as a notifiable disease and the clinical signs include mastitis, arthritis and kerato-conjunctivitis [5]. Contagious agalactia is also caused by several members of the mycoides cluster, including M. mycoides subspecies mycoides Large Colony type and M. capricolum subspecies capricolum [5]. Interestingly, while these mycoplasmas are phylogenetically distant from M. agalactiae, detailed in silico genomic analyses have revealed that extensive horizontal gene transfer has occurred between M. agalactiae and members of the mycoides cluster, and as a result these mycoplasmas may share a number of common cell surface functional domains [3], [6]. Phylogenetically, M. agalactiae is closely related to M. bovis [7], a pathogen of large ruminants that causes clinical signs similar to those of contagious agalactia [8]. For all these ruminant mycoplasmoses, the factors involved in colonization, dissemination and pathogenicity are poorly understood. As a number of genetic tools and genomic data are available for M. agalactiae [6], [9], [10], this species is a useful model for studying the molecular players involved in infectious processes and thus furthering comprehension of pathogenic mechanisms in other mycoplasmas.

A common approach used to identify virulence genes in pathogenic bacteria is based on random transposon mutagenesis [11]–[13]. In mycoplasmas, this approach has mainly been applied to study the minimal set of essential genes [14]–[16], but has also been successfully employed in a few cases to identify genes potentially involved in pathogenicity [17], gliding motility and adherence [18], [19]. Such an approach is needed to further understanding of M. agalactiae, as in silico analyses of currently available ruminant mycoplasma genomes has failed to reveal unambiguously loci that might contribute to infection. Indeed, predicted M. agalactiae gene products have little to no similarity to virulence factors known in other bacteria, and 40% of the coding sequences (CDSs) have been annotated as hypothetical proteins with unknown functions [6]. For M. agalactiae and other ruminant species, one limitation of global transposon mutagenesis to identify virulence genes is the absence of a small laboratory animal model of infection, as in vivo screening in the natural ruminant hosts is constrained by both technical and ethical problems. To overcome these issues, we developed a method for high-throughput screening of M. agalactiae knockout mutants by co-cultivating M. agalactiae mutants with HeLa cells [20]. This assay allowed the selection of a number of genomic regions potentially required for growth in HeLa cell cultures, but dispensable in axenic conditions. Human epithelial surfaces are not a natural environment for M. agalactiae, so we extended our functional genomic study by using two caprine cell lines that are more relevant to the natural host context: goat mammary epithelial cells, TIGMEC, which are likely to be good targets based on the predilection of M. agalactiae for the mammary gland, and goat embryo fibroblasts, TIGEF.

Over 2000 M. agalactiae mutants were co-cultured with caprine cells and those showing a significant reduction in their capacity to grow were examined in detail, revealing 62 loci potentially required for propagation in the host environment. The relevance of these loci and the potential role of the genes at these loci in M. agalactiae-host interactions were analyzed.

Materials and Methods

Bacteria, cell lines and culture conditions

M. agalactiae reference strain PG2 (Refseq NC_009497) [6] was grown in Aluotto or SP4 medium as described previously [20]. Titers were determined by serial dilution in Dulbecco's phosphate-buffered saline (Invitrogen) containing 1% heat-inactivated horse serum (Invitrogen). E. coli DH10B (Invitrogen) was used for DNA cloning and plasmid propagation. The human and caprine cell lines used in this study included HeLa cells (ATCC CCL2), SV40 large T-antigen immortalized goat embryo fibroblasts (TIGEF) and similarly immortalized goat mammary epithelial cells (TIGMEC). TIGMEC were derived from milk epithelial cells [21]. Immortalized cells exhibited morphological and phenotypic features of parental milk epithelial cells and expressed cytokeratin, a specific marker of epithelial cells. Immortalized goat embryo fibroblasts were generated from carpal synovial membrane explants and displayed morphological features of fibroblastic cells [22]. Cells were grown in Dulbecco's modified Eagle's medium (DMEM)-based medium, as described previously [20], composed of DMEM (high glucose, sodium pyruvate, and GlutaMAX-I; Invitrogen) supplemented with non-essential amino acids (NEAA; Invitrogen) and 10% heat-inactivated fetal calf serum (FCS; Eurobio).

M. agalactiae knockout mutant library

The library of knockout mutants was produced in M. agalactiae reference strain PG2 [20]. Transposon mutagenesis was carried out using plasmid pMT85, which does not replicate in mycoplasmas, but contains a modified version of transposon Tn4001 (mini-Tn) conferring gentamicin resistance [23]. Mutants were collected from individual transformations to produce a representative library of 2,175 individual mutants. The pMT85-based library was propagated in SP4 medium supplemented with 500 µg cephalexin/ml (Virbac) and 50 µg gentamicin/ml (Invitrogen). Transposon insertion sites in the M. agalactiae chromosome were mapped by direct sequencing of the junction between the M. agalactiae genomic DNA and the 3′ end of the transposon using BigDye Terminator chemistry and oligonucleotide primer SG8 (Table 1). Direct sequencing was performed at the sequencing facility at the Bio-Medical Research Federative Institute of Toulouse (Toulouse, France). The 3′ end of the mini-Tn was defined using the orientation of the gentamicin resistance gene as the reference [23]. The Pip, MucB and P40 minus mutants were identified by PCR screening of the mutant library using specific oligonucleotide primers [20]. The mutants NifS1 and NifS2 have been described previously as mutants 7.82 and 7.134, respectively [20]. These mutants had a mini-Tn insertion at genomic positions 86804 (Pip), 88958 (MucB), 281483 (P40 minus), 87172 (NifS1) or 88125 (NifS2). The mini-Tn gentamicin resistance gene in the NifS1, Pip, MucB and P40 minus mutants was in the opposite orientation compared to the disrupted CDS, but in the same orientation in the NifS2 mutant.

Table 1

Oligonucleotides used in this study.

High-throughput screening of M. agalactiae knockout mutant library in cell culture

A cell-culture assay was used to screen the M. agalactiae knockout mutant library and identify mutants displaying a growth-deficient phenotype [20]. Briefly, cells seeded in 96-well plates were inoculated with cultures of individual mutants using a 96-pin replicator (Boekel Scientific). Growth-deficient mutants were selected based on the titers reached at the end of the co-cultivation period. After one freeze-thaw cycle (−80°C/+37°C), co-cultures were spotted onto solid medium using a 96-pin replicator. The development of mycoplasma colonies was used as a cut-off point (Table 2). Culture stocks (inoculum) of M. agalactiae knockout mutants were tested by direct spotting onto solid medium. The titer reached by the wild-type after co-cultivation with HeLa cells [20], TIGMEC or TIGEF cells was not influenced by variations in the initial inoculum size (data not shown). M. agalactiae was unable to proliferate in cell-culture medium alone [20].

Table 2

High-throughput detection of M. agalactiae mutants unable to grow on cultured cells.

RNA extraction, RT-PCR amplification and primer extension

Total RNA was extracted from 48 hour cultures of M. agalactiae using the TRIzol method (Invitrogen). RNA samples were stored at −80°C. The RNA concentration was determined spectrophotometrically by measuring absorbance at 260 nm and by agarose gel electrophoresis. RT-PCRs were carried out with the Access RT-PCR System kit (Promega), using 1 µg of total RNA treated with DNAse (RNase-free DNAse, Promega). Reactions were incubated at 45°C for 45 min, 94°C for 2 min, then through 30 cycles of 94°C for 30 sec, 56°C for 1 min and 72°C for 30 sec, with a final extension incubation of 7 min at 72°C. Amplification products were analyzed by agarose gel electrophoresis. Primer extension was carried out using 15 µg of total RNA, 2 pmol of the labeled oligonucleotide primer 5′-6FAM-NifS1 (Table 1), and 200 units of Superscript III Reverse Transcriptase (Invitrogen). RNAs were denatured by 5 min incubation at 65°C. Reverse transcription reactions were performed at 42°C for 50 min, followed by enzyme inactivation at 75°C for 15 min. The cDNAs were treated with RNAse A (Promega) for 30 min at 37°C, ethanol precipitated and resuspended in 10 µl formamide and 0.4 µl of GS-400HD ROX size standards (Applied Biosystems). Product sizes were analyzed using the ABI3730 sequencer (Applied BioSystems) at the GenoToul genomic platform of Toulouse (France).

A reporter system for the detection of transcriptional promoter sites in M. agalactiae

The surface antigen P40 CDS MAG2410 was used as a reporter gene to assess transcriptional promoter activity in M. agalactiae. DNA sequences to be tested were cloned upstream of CDS MAG2410 using the plasmid p20-1miniO/T as a vector [20]. The 3′ end of the pip gene was amplified by PCR using the primers Pip-86804_F and Pip-P40_R (Table 1) to generate a 191 bp fragment overlapping CDS MAG2410. CDS MAG2410 was amplified using Pip-P40_F and CCP40-03 (Table 1) to generate a 1188 bp fragment overlapping the 3′ end of the pip gene. The two overlapping fragments were assembled by PCR amplification using the primers Pip-86804_F and CCP40-03 (Table 1). The resulting PCR products were cloned into the pGEM-T Easy vector (Promega), before sub-cloning into the NotI site of plasmid p20-1miniO/T. PCR amplifications were performed using the proofreading Phusion High Fidelity polymerase (Finnzymes). Before cloning into pGEM-T Easy, 3′-terminal deoxyadenosine residues were added to blunt-ended PCR products by following the A-tailing procedure provided by the supplier (Promega). Cloned sequences were verified by DNA sequencing. CDS MAG2410 alone or with its own promoter sequence was used as negative and positive controls, respectively. PCR amplifications were performed using primers P40_RF_CC and CCP40-03 (positive control), and Pip-P40_F and CCP40-03 (negative control)(Table 1).

A surface antigen P40-knockout mutant (P40 minus; see above) was used to test the expression of P40 from the different plasmid constructs. M. agalactiae cells (10⁸ to 10⁹ CFU) were transformed by electroporation using 1 to 3 µg of plasmid DNA, as described previously [20]. After 3 hours incubation in non-selective medium, cells were allowed to grow in the presence of appropriate antibiotic for 24 hours before plating on selective solid medium. Transformants were picked after 4 to 7 days and subcultured in selective SP4 medium. The expression of M. agalactiae surface antigen P40 was tested by Western blotting.

Western blotting and immunodetection of M. agalactiae lipoprotein P40

Mycoplasmas grown in SP4 medium were collected by centrifugation at 10,000× g and resuspended in Dulbecco's phosphate-buffered saline (Invitrogen). The protein concentration was determined using the Quick Start Bradford protein assay (Bio-Rad). For Western blotting, total proteins (0.5 µg) were separated by SDS-PAGE using the Mini-Protean II electrophoresis system (Bio-Rad) and transferred to Protran nitrocellulose membranes (Whatman). Membranes were blocked in Tris-buffered saline (TBS) (10 mM TrisHCl, pH 7.4; 150 mM NaCl) containing 5% skim milk for 2 hours, then incubated overnight at 4°C with a sheep anti-P40 serum at a dilution of 1/500 in TBS containing 0.05% Tween 20 and 10% heat-inactivated horse serum (Invitrogen). Western blots were developed using horseradish peroxidase conjugated secondary antibody raised in rabbits (DAKO) and 4-chloro-naphthol as substrate. Sheep serum raised against the M. agalactiae surface antigen P80 was used as a control (dilution of 1/200). The anti-P40 and anti-P80 sheep sera were produced by animal immunization with P40 or P80 recombinant proteins, respectively (data not shown).

Results and Discussion

High-throughput identification of M. agalactiae growth-deficient mutants upon co-cultivation with host cells

Our group has previously reported the construction of a library of M. agalactiae knockout mutants together with the development of a high-throughput screening method based on the co-cultivation of M. agalactiae mutants with HeLa cells [20]. Since human epithelial cells are not a natural environment for M. agalactiae, we subsequently screened the library with two caprine cell lines, which are likely to be more relevant to the normal host-cell interactions involved in infections with this pathogen. The goat mammary epithelial cells, TIGMEC, are likely to be particularly relevant given the predilection of M. agalactiae for the mammary gland. HeLa cells were used as a control.

The ability of individual mutants to grow in the presence of these three cell lines was assessed after 3 days of co-cultivation by directly spotting the cultures onto solid medium and comparing the titers (see Materials and Methods). A total of 209 growth-deficient mutants were selected out of 2,175 tested, using a cut-off value of 10 colonies per plate, which corresponded to a titer of 10⁵ CFU/ml in co-cultures (Table 2). The mutants unable to grow in each cell line are shown in Fig. 1A, with a detailed description of those unable to grow on caprine cells provided in Tables 3 and and4.4. Some differences were seen between the repertoire of mutants identified as growth deficient on HeLa cells in the current study and those identified in our previous study [20], with only 61% common to both studies. This reflects the limitations of these assays, including some cross contamination between individual mutants stored in 96-well plates. These were found to hamper the selection of mutants with reduced growth capacities in cell culture (data not shown) and to affect the reproducibility of the screening from one experiment to the other.

Figure 1

Overall distribution of M. agalactiae growth deficient mutants selected after co-cultivation with host cells.

Table 3

M. agalactiae CDSs identified by high-throughput screening for their reduced growth capacities on cultured cells.

Table 4

M. agalactiae NCRs identified by high-throughput screening with host cells.

Some mutants (27%) displayed reduced growth capacities on multiple cell types, while the majority (73%) exhibited this phenotype on one cell line (Fig. 1A). Interestingly, only a small number of mutants were selected on TIGMEC, compared to the number selected on TIGEF and HeLa cells (Table 2). It is possible that the tolerance of M. agalactiae to transposon mutagenesis increases when grown on a cell type similar to its natural environment, but this hypothesis needs to be confirmed with a larger panel of host cell types.

Mapping of transposon insertion sites in the genome of growth-deficient M. agalactiae mutants

Direct genomic sequencing was performed to determine the position of the transposon in mutants found to be inhibited on caprine cell lines. The 110 mutants had 62 unique insertion sites that mapped within 46 different coding sequences (CDS) and 9 non-coding regions (NCR) (Fig. 1B and Tables 3, ,4).4). The examination of DNA sequence chromatograms failed to reveal multiple transposon insertion events in the M. agalactiae chromosome (data not shown).

As shown in Figure 1C, most of the disrupted CDSs have been annotated as hypothetical proteins (HP) of unknown function (no COG). Within this category, predicted surface lipoproteins were highly represented 2.1 times more than would be expected [6]. Because of the absence of a cell wall in mycoplasmas, cell surface lipoproteins are thought to be key players in modulating interactions with the host. Interestingly, 20 mutants with a disruption in the same lipoprotein gene (MAG2540) were inhibited on the TIGEF, but not the TIGMEC (Table 3). All had the transposon inserted at the same position, suggesting that they were probably siblings derived from the same parental clone. The repeated selection of this particular mutant suggests a role for MAG2540 in the proliferation of M. agalactiae on TIGEF, even though it is dispensable in axenic culture medium and in the presence of TIGMEC. The function of this CDS is unknown, but it is predicted to encode a surface lipoprotein (Vpma-like lipoprotein) with similarities to some domains of the hypervariable Vpma lipoproteins of M. agalactiae [24]. Because MAG2540 knockout mutants were also repeatedly selected on HeLa cells, it is possible that, in the absence of specific receptors on target cells such as the TIGMEC, this Vpma-like lipoprotein facilitates binding to ubiquitous structures on mammalian cell surfaces. This implies that growth of M. agalactiae in cell cultures requires a close interaction with the cells that is lost in the MAG2540 knockout mutants when growing on TIGEF or HeLa cells. As expected for bacteria with small genomes and reduced metabolic pathways, “transport and metabolism” (COG categories E, F, G, H and P) was the largest functional category involved in interactions between M. agalactiae and caprine cells, with 17% of the mutants selected having insertions in genes involved in these functions (Fig. 1C). Since the wild-type is unable to proliferate in cell-culture medium alone [20], it is most likely that these mutants are unable to transport or metabolize some of essential nutrients provided by the cultured cells. The remaining CDSs for which a predicted function had been assigned were distributed across a broad range of functional categories (Fig. 1C), often without any predictable correlation with their role in interactions with caprine cells.

Some of the loci identified in mutants selected on caprine cell lines (Tables 3 and and4),4), were also identified as being required for growth on HeLa cells, either in this study (Tables 3 and and4)4) or in our previous study [20]. This suggests that these loci may be involved in general processes mediating interactions between M. agalactiae and mammalian cells. The functions encoded by several of these, including DNA repair (uvrA), nucleotide metabolism (apt), iron-sulfur cluster biosynthesis (nifS), and protein folding (tig), contribute to stress tolerance and virulence in a number of pathogenic bacteria [25]–[31].

A global proteomic analysis of gene products expressed by M. agalactiae strain PG2 in axenic culture [32] detected approximately 50% of the CDSs found to be required for growth on caprine cells (Table 3). Whether this reflects the limited sensitivity of the proteomic approach, or differential expression by M. agalactiae under axenic and co-culture conditions is not known.

About 20% of the mutants selected on caprine cells had an insertion in a NCR (Table 4). The importance of NCRs in the biology of M. agalactiae remains largely unexplored, but several are likely to include transcriptional promoters and other regulatory regions. Re-examination of the 9 mutated NCRs using the AMIGene annotation tool [33] revealed that two, NCR E and G, had an insertion within short CDSs (Table 4) that had not been annotated previously but that could encode products with a role in host-cell interaction. Interestingly, transcriptional activity in NCRs has been reported for a number of mycoplasmas [34], [35], suggesting an active role for these regions. NCRs D, E and F (Table 4) are part of a 20 kb locus containing a vestige of an integrative conjugative element (ICEA) [6], [36]. The mechanism by which NCRs may regulate the proliferation of M. agalactiae in cell culture remains to be elucidated.

Finally, several CDSs required for growth on host cells are conserved in other ruminant mycoplasma species, and/or were involved in the massive horizontal gene transfer (HGT) that occurred between M. agalactiae, M. bovis and members of the phylogenetically distant mycoides cluster (Table S1). Two CDSs (MAG2870 and MAG6690) were also predicted to have undergone HGT between the avian mycoplasma species M. synoviae and M. gallisepticum (Table S1). About 70% of these CDSs involved in HGT encode membrane-associated proteins, and thus are likely to play a role in mycoplasma–host interactions. The genome-scale analysis of M. agalactiae in cell culture may assist in understanding pathogenic processes involved in other mycoplasma infections.

The frequent occurrence of promoter regions in the genome of M. agalactiae reduces polar effects mediated by integrated transposon sequences

As mentioned above, some CDSs required for growth on cell cultures fell into functional categories (Fig. 1C) that had no obvious correlation with mycoplasma-host interactions. This raised the question of whether growth-deficient phenotypes can result from a polar downstream effect rather than the effect on the gene disrupted by the transposon insertion. The compact mycoplasma genome, which is often organized into highly dense co-linear gene clusters with operon-like structures, suggests that this might be likely [3].

To evaluate the potential influence of the mini-Tn insertions on gene expression from these operon-like structures, we analyzed the 4 kb co-linear gene cluster pip-nifS-nifU-mucB (MAG0710 to MAG0740) (Fig. 2). This cluster was of particular interest because: (i) nifS has been shown to be essential for proliferation of M. agalactiae on cell cultures, and two knockout mutants, NifS1 and NifS2, were identified by high-throughput screening on caprine and human cells (Table 3); and (ii) these co-linear genes are likely to be co-transcribed by a promoter located upstream of pip, based on genome data indicating short intergenic distances (Fig. 2A). Indeed, the operon-like structure of the pip-nifS-nifU-mucB cluster was further supported by our transcriptional analyses, which detected overlapping transcripts by RT-PCR (Fig. 2A). Two mutants, Pip and MucB, with a transposon inserted into the corresponding genes, were searched for and found in the mutant library (see Materials and Methods), but both are able to grow on all three cell lines. When tested individually with TIGMEC, both mutants had the wild-type phenotype (Fig. 2B). This result was surprising, at least for the Pip mutant, which was expected to have a similar phenotype to that of the NifSs mutants because of the predicted polar effect of the transposon insertion (Fig. 2A).

Figure 2

The nif locus in M. agalactiae is a promoter-less CDS cluster inserted within a transcriptionally active region.

RT-PCR amplification using oligonucleotide primers bracketing the mini-Tn integration site in mutants Pip, NifS1, and NifS2 did not detect mRNA (RT-PCR II in mutants Pip and NifS1, and RT-PCR IV in mutant NifS2), but, unexpectedly, transcripts were detected downstream of the mini-Tn (RT-PCR III and IV in mutants Pip and NifS1), suggesting that there may be a promoter within pip or the mini-Tn. The presence of a promoter within the integrated mini-Tn sequences was suggested by the identification of RNA transcripts that overlapped the 3′ end of the mini-Tn and nifS in Pip and NifS1 mutants (data not shown). The extension of transcription beyond the 3′ end of the mini-Tn was probably responsible for the expression of downstream genes in knockout mutants of M. agalactiae and may have influenced the orientation of the mini-Tn in the mutant library [20]. Although promoter sequences in the mini-Tn remain to be formally demonstrated, constitutive gene expression from the 3′ end of the mini-Tn can also be viewed as another outcome of transposon mutagenesis. Experiments are in progress to determine the role of this mechanism in mutants unable to grow in cell cultures that harbor a transposon within a NCR.

Recent studies on Mycoplasma genitalium have revealed that the genome of this human pathogen is actively transcribed, and contains multiple cryptic promoters [34]. This led us to further explore transcriptional activity within the pip-nifS-nifU-mucB cluster, and to examine the promoter activity at the 3′ end of the pip gene. A reporter system was developed to detect promoter sequences in M. agalactiae (Fig. 2C). Lipoprotein P40 (MAG2410) is a surface antigen of M. agalactiae, the expression of which can be detected using specific antibodies. The successful complementation of a M. agalactiae mutant, P40 minus, harboring a transposon within the P40 lipoprotein gene, with a plasmid expressing P40, led us to develop a reporter system to detect promoter activity. Western blotting analyses confirmed that the 157 nucleotides at the 3′ end of the pip gene, when inserted at the 5′ end of the P40 lipoprotein gene, promote complementation of the P40 minus mutant.

Finally, the transcriptional start point at the 3′ end of the pip gene was mapped by primer extension using the oligonucleotide 5′-6FAM-NifS1 (Table 1). A major extension product with a size of between 163 and 165 nucleotides was obtained, indicating that the transcriptional start point was 31 nucleotides upstream of the stop codon of the pip gene (Fig. 2D). The detection of multiple extension products differing in length by a single nucleotide is a common finding in mycoplasma promoters [34], [37].

The genomes of mycoplasmas are characterized by a low G+C content. This particular feature may favor the occurrence of primary or secondary promoter regions in the genome of M. agalactiae, even within coding sequences such as this promoter within the 3′ end of the pip gene. The high density of promoters within the genome of M. agalactiae may have important evolutionary consequences, facilitating chromosomal rearrangements and gene shuffling in these rapidly evolving organisms.

Gene involved in the interaction of M. agalactiae with host cells may have been hitchhiking across evolution

Although polar effects resulting from the disruption of co-transcribed gene clusters cannot be ruled out, the identification of multiple transposon insertion sites in the same region suggests that important factors mediating the interaction between M. agalactiae and host cells may map to these loci. Among the 62 loci identified after screening with host cells, six loci mutants had insertions in the same CDS or NCR, but at different positions (Tables 3 and and4).4). CDSs with multiple insertion sites included two HP predicted to be exposed on the cell surface (MAG1430 and MAG2870), and cytosolic proteins with homologies with cysteine desulfurase (MAG0720), the P115-like ABC transporter ATP binding protein (MAG4380), and DNA polymerase III subunits gamma and tau (MAG6870). Only one NCR (NCR I) was found containing two different insertions that inhibited the capacity of M. agalactiae to grow on host cells. Interestingly, CDSs MAG0720 (nifS) and MAG6870 (dnaX) each belong to co-linear gene clusters (Fig. 3) that are highly conserved in Mollicutes (Fig. S1, S2, and S3). The remarkable conservation of these two gene clusters led us to examine the co-localization of the 46 CDS identified as being required for growth of M. agalactiae on cultured cells, and to compare the synteny of these CDSs using complete genome sequences of mycoplasmas available in public databases. A total of 8 highly conserved co-linear gene clusters were identified (Fig. 3 and Fig. S1, S2, and S3). Several of these clusters encode proteins predicted to be involved in specific functions, including [Fe-S] cluster biosynthesis (NIF), chromate transport (CHR), cell division (MRAZ) and DNA replication, recombination and repair (DNAX). The potential role of these CDS clusters in the interaction between M. agalactiae and host cells was further supported by the similar effect of transposon insertions at different positions in these CDS clusters (NIF, PKNB, MRAZ, CHR and DNAX in Fig. 3). The essential role of the NIF locus in the interaction between M. agalactiae and host cells has been demonstrated previously by complementation studies [20].

Figure 3

Genomic loci carrying transposon insertions in M. agalactiae mutants displaying reduced growth capacities in cell culture.

The location of these CDS clusters can differ considerably from one mycoplasma species to another, even within the same phylogenetic group (Fig. S1, S2, and S3). In M. agalactiae, promoter sequences initiating the transcription of nifS were located outside of the NIF locus, with a sequence identified within the 3′ end of the pip gene (see above). Interestingly, the pip gene does not always co-localize with the NIF locus in other mycoplasma species, suggesting that this locus is inserted within transcriptionally active regions. Thus, it is tempting to speculate that some of the genes involved in the interaction between M. agalactiae and host cells may have been hitchhiking across evolution for transcriptionally active regions of the mycoplasma chromosome. Further evidence is needed to support this hypothesis.

In conclusion, cell culture provides a simple and efficient screening system for genome-scale analysis of mycoplasma loci contributing to host-pathogen interactions. This global approach, when combined with in vivo studies, can be an efficient strategy for identifying key factors involved in mycoplasma virulence and host-colonization, as well as a way to understand pathogenic processes involved in disease caused by these unconventional pathogens. The absence of small animal models for M. agalactiae and other ruminant mycoplasmal pathogens has been a significant bottleneck for functional genomics studies using large mutant libraries. High-throughput screening of more than 2000 individual clones by co-culture with host cells revealed 62 loci in the genome of M. agalactiae that were required for growth in this environment. The relevance of these loci in the biology of M. agalactiae when it replicates in its natural host remains to be determined, but experimental infections in lactating ewes have confirmed the essential role played by nifS in host-colonization (data not shown). Since the specific cell line was shown to influence which mutants were selected, comparative studies with different cell types, including differentiated monolayer cultures and cellular players involved in the immune response to infection, may provide further information about the interactions of mycoplasmas in these different cellular environments. Finally, these results provide an experimental framework for the development of control strategies, based on attenuated live vaccines, against mycoplasmosis in ruminant species.

Supporting Information

Figure S1

Genomic position of short CDS clusters NIF, HPRK, MRAZ and CHR in mycoplasma species with sequenced genomes. Gene organization of the conserved CDS clusters identified during the screening was analyzed using the Microbial Genome Database for Comparative Analysis software [40]. Homologues genes are indicated by the same color code and a black bar. Three examples were chosen for each phylogenetic group. In the case of the CHR locus, no homolog was identified in the Pneumoniae group. MA: M. agalactiae, MMOB: M. mobile, MYPU: M. pulmonis, MLEA: M. leachii, MmmSC: Mycoplasma mycoides subsp. mycoides SC, MCAP: M. capricolum subsp. capricolum, UPAR: U. parvum, UURE: U. urealyticum, MGAL: M. gallisepticum.

(TIF)

Click here for additional data file.^{(378K, tif)}

Figure S2

Genomic position of short CDS clusters PKNB and ATP in mycoplasma species with sequenced genomes. Gene organization of the conserved CDS clusters identified during the screening was analyzed using the Microbial Genome Database for Comparative Analysis software [40]. Homologues genes are indicated by the same color code and a black bar. Three examples were chosen for each phylogenetic group. MA: M. agalactiae, MMOB: M. mobile, MYPU: M. pulmonis, MLEA: M. leachii, MmmSC: Mycoplasma mycoides subsp. mycoides SC, MCAP: M. capricolum subsp. capricolum, UPAR: U. parvum, UURE: U. urealyticum, MGAL: M. gallisepticum.

(TIF)

Click here for additional data file.^{(269K, tif)}

Figure S3

Genomic position of short CDS clusters DNAX and SCPB in mycoplasma species with sequenced genomes. Gene organization of the conserved CDS clusters identified during the screening was analyzed using the Microbial Genome Database for Comparative Analysis software [40]. Homologues genes are indicated by the same color code and a black bar. Three examples were chosen for each phylogenetic group. MA: M. agalactiae, MMOB: M. mobile, MYPU: M. pulmonis, MLEA: M. leachii, MmmSC: Mycoplasma mycoides subsp. mycoides SC, MCAP: M. capricolum subsp. capricolum, UPAR: U. parvum, UURE: U. urealyticum, MGAL: M. gallisepticum.

(TIF)

Click here for additional data file.^{(317K, tif)}

Table S1

Degree of homology of CDS disrupted in M. agalactiae mutants with other ruminant mycoplasma species. ^aCDS found disrupted in M. agalactiae growth-deficient mutants [6]. ^bHypothetical proteins (HP) have no homolog outside the M. agalactiae species. Conserved hypothetical proteins (CHP) share sequence similarity with proteins of unknown function identified in mollicutes or other bacteria. COG categories of encoded proteins are indicated in parenthesis [38]. ^cProtein localization was predicted using TMHMM [40]; membrane (M), cytosolic (C), or indirectly linked to the membrane (IM). ^dGenes supposed to have undergone horizontal gene transfer (HGT) between M. agalactiae and mycoplasmas from the mycoides cluster [6] are indicated by a plus sign (+). Genes displaying homologies with sequences in M. gallisepticum or M. synoviae genomes and supposed to have undergone HGT between these two species are identified by a cross sign (x) [6]. ^ePercentages of identity and similarity were determine by local BLAST using Molligen [42]. ^fMCAP stands for M. capricolum subsp. capricolum.

(DOC)

Click here for additional data file.^{(119K, doc)}

Acknowledgments

We thank Dr. J. Frey (University of Bern, Switzerland) for providing the P40 recombinant protein and Dr. P. Giammarinaro (GDS64, Pau, France) for his help in producing the anti-P80 sheep serum. We also thank Dr. C. Leroux (INRA, Lyon, France) for providing the TIGMEC and TIGEF cell lines.

Footnotes

Competing Interests: The authors have declared that no competing interests exist.

Funding: This work was supported by a joint grant from INRA (www.inra.fr) and CIRAD (www.cirad.fr) and by a doctoral fellowship to AS from INRA and DGER (www.envt.fr). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

References

1. Edward DGF, Freundt EA, Chanock RM, Fabricant J, Hayflick L, et al. Recommendations on nomenclature of the order Mycoplasmatales. Science. 1967;155:1694–1696. [PubMed]

2. Razin S, Yogev D, Naot Y. Molecular biology and pathogenicity of mycoplasmas. Microbiol Mol Biol Rev. 1998;62:1094–1156. [PMC free article] [PubMed]

3. Sirand-Pugnet P, Citti C, Barré A, Blanchard A. Evolution of Mollicutes: down a bumpy road with twists and turns. Res Microbiol. 2007;158:754–766. [PubMed]

4. Frey J. Molecular biology and pathogenicity of mycoplasmas. New York (USA): S. Razin and R. Herrmann; 2002. Mycoplasmas of animals. pp. 73–90.

5. Bergonier D, Berthelot X, Poumarat F. Contagious agalactia of small ruminants: current knowledge concerning epidemiology, diagnosis and control. Rev Off Int Epizoot. 1997;16:848–873. [PubMed]

6. Sirand-Pugnet P, Lartigue C, Marenda M, Jacob D, Barré A, et al. Being pathogenic, plastic, and sexual while living with a nearly minimal bacterial genome. PLoS Genet. 2007;3:e75. [PubMed]

7. Pettersson B, Uhlén M, Johansson KE. Phylogeny of some mycoplasmas from ruminants based on 16S rRNA sequences and definition of a new cluster within the hominis group. Int J Syst Bacteriol. 1996;46:1093–1098. [PubMed]

8. Pfützner H, Sachse K. Mycoplasma bovis as an agent of mastitis, pneumonia, arthritis and genital disorders in cattle. Rev Off Int Epizoot. 1996;15:1477–1494. [PubMed]

9. Chopra-Dewasthaly R, Marenda M, Rosengarten R, Jechlinger W, Citti C. Construction of the first shuttle vectors for gene cloning and homologous recombination in Mycoplasma agalactiae. FEMS Microbiol Lett. 2005;253:89–94. [PubMed]

10. Chopra-Dewasthaly R, Zimmermann M, Rosengarten R, Citti C. First steps towards the genetic manipulation of Mycoplasma agalactiae and Mycoplasma bovis using the transposon Tn4001mod. Int J Med Microbiol. 2005;294:447–453. [PubMed]

11. Saenz HL, Dehio C. Signature-tagged mutagenesis: technical advances in a negative selection method for virulence gene identification. Curr Opin Microbiol. 2005;8:612–619. [PubMed]

12. Mazurkiewicz P, Tang CM, Boone C, Holden DW. Signature-tagged mutagenesis: barcoding mutants for genome-wide screens. Nat Rev Genet. 2006;7:929–939. [PubMed]

13. Burrack LS, Higgins DE. Genomic approaches to understanding bacterial virulence. Curr Opin Microbiol. 2007;10:4–9. [PubMed]

14. Hutchison CA, Peterson SN, Gill SR, Cline RT, White O, et al. Global transposon mutagenesis and a minimal Mycoplasma genome. Science. 1999;286:2165–2169. [PubMed]

15. Glass JI, Assad-Garcia N, Alperovich N, Yooseph S, Lewis MR, et al. Essential genes of a minimal bacterium. Proc Natl Acad Sci U S A. 2006;103:425–430. [PubMed]

16. French CT, Lao P, Loraine AE, Matthews BT, Yu H, et al. Large-scale transposon mutagenesis of Mycoplasma pulmonis. Mol Microbiol. 2008;69:67–76. [PMC free article] [PubMed]

17. Hudson P, Gorton TS, Papazisi L, Cecchini K, Frasca S, Jr, et al. Identification of a virulence-associated determinant, dihydrolipoamide dehydrogenase (lpd), in Mycoplasma gallisepticum through in vivo screening of transposon mutants. Infect Immun. 2006;74:931–939. [PMC free article] [PubMed]

18. Hasselbring BM, Page CA, Sheppard ES, Krause DC. Transposon mutagenesis identifies genes associated with Mycoplasma pneumoniae gliding motility. J Bacteriol. 2006;188:6335–6345. [PMC free article] [PubMed]

19. Mudahi-Orenstein S, Levisohn S, Geary SJ, Yogev D. Cytadherence-deficient mutants of Mycoplasma gallisepticum generated by transposon mutagenesis. Infect Immun. 2003;71:3812–3820. [PMC free article] [PubMed]

20. Baranowski E, Guiral S, Sagne E, Skapski A, Citti C. Critical role of dispensable genes in Mycoplasma agalactiae interaction with mammalian cells. Infect Immun. 2010;78:1542–1551. [PMC free article] [PubMed]

21. Mselli-Lakhal L, Guiguen F, Fornazero C, Favier C, Durand J, et al. Immortalized goat milk epithelial cell lines replicate CAEV at high level. Vet Res. 2001;32:12. [PubMed]

22. Da Silva Teixeira MF, Lambert V, Mselli-Lakahl L, Chettab A, Chebloune Y, et al. Immortalization of caprine fibroblasts permissive for replication of small ruminant lentiviruses. Am J Vet Res. 1997;58:579–584. [PubMed]

23. Zimmerman CU, Herrmann R. Synthesis of a small, cysteine rich, 29 amino acids long peptide in Mycoplasma pneumoniae. FEMS Microbiol Lett. 2005;253:315–321. [PubMed]

24. Citti C, Nouvel L-X, Baranowski E. Phase and antigenic variation in mycoplasmas. Future Microbiol. 2010;5:1073–1085. [PubMed]

25. Wen ZT, Suntharaligham P, Cvitkovitch DG, Burne RA. Trigger factor in Streptococcus mutans is involved in stress tolerance, competence development, and biofilm formation. Infect Immun. 2005;73:219–225. [PMC free article] [PubMed]

26. Huet G, Daffe M, Saves I. Identification of the Mycobacterium tuberculosis SUF machinery as the exclusive mycobacterial system of [Fe-S] cluster assembly: evidence for its implication in the pathogen's survival. J Bacteriol. 2005;187:6137–6146. [PMC free article] [PubMed]

27. Bigot A, Botton E, Dubail I, Charbit A. A homolog of Bacillus subtilis trigger factor in Listeria monocytogenes is involved in stress tolerance and bacterial virulence. Appl Environ Microbiol. 2006;72:6623–6631. [PMC free article] [PubMed]

28. Singh A, Guidry L, Narasimhulu KV, Mai D, Trombley J, et al. Mycobacterium tuberculosis WhiB3 responds to O₂ and nitric oxide via its [4Fe-4S] cluster and is essential for nutrient starvation survival. Proc Natl Acad Sci U S A. 2007;104:11562–11567. [PubMed]

29. Runyen-Janecky L, Daugherty A, Lloyd B, Wellington C, Eskandarian H, et al. Role and regulation of iron-sulfur cluster biosynthesis genes in Shigella flexneri virulence. Infect Immun. 2008;76:1083–1092. [PMC free article] [PubMed]

30. Rincon-Enriquez G, Crété P, Barras F, Py B. Biogenesis of Fe/S proteins and pathogenicity: IscR plays a key role in allowing Erwinia chrysanthemi to adapt to hostile conditions. Mol Microbiol. 2008;67:1257–1273. [PubMed]

31. Ambur OH, Davidsen T, Frye SA, Balasingham SV, Lagesen K, et al. Genome dynamics in major bacterial pathogens. FEMS Microbiol Rev. 2009;33:453–470. [PMC free article] [PubMed]

32. Nouvel LX, Sirand-Pugnet P, Marenda MS, Sagné E, Barbe V, et al. Comparative genomic and proteomic analyses of two Mycoplasma agalactiae strains: clues to the macro- and micro-events that are shaping mycoplasma diversity. BMC Genomics. 2010;11:86. [PMC free article] [PubMed]

33. Bocs S, Cruveiller S, Vallenet D, Nuel G, Médigue C. AMIGene: Annotation of MIcrobial Genes. Nucleic Acids Res. 2003;31:3723–3726. [PMC free article] [PubMed]

34. Lluch-Senar M, Vallmitjana M, Querol E, Piñol J. A new promoterless reporter vector reveals antisense transcription in Mycoplasma genitalium. Microbiology. 2007;153:2743–2752. [PubMed]

35. Gardner SW, Minion FC. Detection and quantification of intergenic transcription in Mycoplasma hyopneumoniae. Microbiology. 2010;156:2305–2315. [PubMed]

36. Marenda M, Barbe V, Gourgues G, Mangenot S, Sagne E, et al. A new integrative conjugative element occurs in Mycoplasma agalactiae as chromosomal and free circular forms. J Bacteriol. 2006;188:4137–4141. [PMC free article] [PubMed]

37. Weiner J, Herrmann R, Browning GF. Transcription in Mycoplasma pneumoniae. Nucleic Acids Res. 2000;28:4488–4496. [PMC free article] [PubMed]

38. Tatusov RL, Koonin EV, Lipman DJ. A genomic perspective on protein families. Science. 1997;278:631–637. [PubMed]

39. Rutherford K, Parkhill J, Crook J, Horsnell T, Rice P, et al. Artemis: sequence visualization and annotation. Bioinformatics. 2000;16:944–945. [PubMed]

40. Uchiyama I. MBGD: microbial genome database for comparative analysis. Nucleic Acids Res. 2003;31:58–62. [PMC free article] [PubMed]

41. Krogh A, Larsson B, von Heijne G, Sonnhammer EL. Predicting transmembrane protein topology with a hidden Markov model: application to complete genomes. J Mol Biol. 2001;305:567–580. [PubMed]

42. Barré A, de Daruvar A, Blanchard A. MolliGen, a database dedicated to the comparative genomics of Mollicutes. Nucleic Acids Res. 2004;32:D307–10. [PMC free article] [PubMed]

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