http://orcid.org/0000-0002-8390-8123
Figures
Abstract
Release of extracellular vesicles (EV) by Gram-negative and positive bacteria is being frequently reported. EV are nano-sized, membrane-derived, non-self-replicating, spherical structures shed into the extracellular environment that could play a role in bacteria-host interactions. Evidence of EV production in bacteria belonging to the class Mollicutes, which are wall-less, is mainly restricted to the genus Acholeplasma and is scanty for the Mycoplasma genus that comprises major human and animal pathogens. Here EV release by six Mycoplasma (sub)species of clinical importance was investigated. EV were obtained under nutritional stress conditions, purified by ultracentrifugation and observed by electron microscopy. The membrane proteins of EV from three different species were further identified by mass spectrometry as a preliminary approach to determining their potential role in host-pathogen interactions. EV were shown to be released by all six (sub)species although their quantities and sizes (30–220 nm) were very variable. EV purification was complicated by the minute size of viable mycoplasmal cells. The proteins of EV-membranes from three (sub)species included major components of host-pathogen interactions, suggesting that EV could contribute to make the host-pathogen interplay more complex. The process behind EV release has yet to be deciphered, although several observations demonstrated their active release from the plasma membrane of living cells. This work shed new light on old concepts of “elementary bodies” and “not-cell bound antigens”.
Citation: Gaurivaud P, Ganter S, Villard A, Manso-Silvan L, Chevret D, Boulé C, et al. (2018) Mycoplasmas are no exception to extracellular vesicles release: Revisiting old concepts. PLoS ONE 13(11): e0208160. https://doi.org/10.1371/journal.pone.0208160
Editor: Catherine A. Brissette, University of North Dakota School of Medicine and Health Sciences, UNITED STATES
Received: September 28, 2018; Accepted: November 13, 2018; Published: November 28, 2018
Copyright: © 2018 Gaurivaud 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.
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: Sarah Ganter’s PhD research is jointly funded by the French Agency for Food, Environmental and Occupational Health and Safety (Anses) and the French Agricultural Research Centre for International Development (CIRAD). The funder had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Introduction
Extracellular vesicles (EV) are nano-sized, membrane-derived, non-self-replicating, spherical structures shed into the extracellular environment by both eukaryotic and prokaryotic cells [1]. Most prokaryotic EV studied since the earliest observations in the 1960s [2] are Gram-negative outer membrane vesicles [3]. Their composition, biogenesis and role in bacterial virulence and cross-talk with eukaryotic cells have been deciphered in various bacterial models [4]. In contrast, EV from Gram-positive bacteria have been poorly characterized up to now even though they were first observed by electron microscopy in a Bacillus culture as early as 1990 [5]. The first characterization of EV released by a Gram-positive bacteria came from the seminal study of Staphylococcus aureus in 2009 [6] and, since then, EV have been described in several Gram-positive genera, such as Bacillus, Streptomyces, Listeria, Clostridium and Streptococcus [7–11]. In the absence of an outer membrane, Gram-positive EV are formed from the cytoplasmic membrane. Hence the thick peptidoglycan cell wall is certainly a physical barrier that could hinder their release and explain the low yield of EV production from Gram-positive bacteria in vitro [12].
Within the Gram-positive phylum, bacteria belonging to the class Mollicutes hold a special place as they are wall-less, minute-sized cells limited only by a cytoplasmic membrane. They evolved from a common Gram-positive ancestor with a low G+C content and are phylogenetically close to Clostridium spp. [13]. The genetic relatedness with the EV-producing Clostridium genus [7] and the lack of a cell wall physical barrier are two reasons why we could expect EV production from Mollicutes. This was indeed demonstrated by Chernov and collaborators in 2011 using Acholeplasma (A.) laidlawii as a model [14]. A. laidlawii is a filament-shaped mollicute (0.5 μm wide, 2.0 μm long [15]), widespread in nature. The EV observed by electron microscopy from a culture grown under starvation conditions were 70 to 120 nm in length [14] and contained DNA, RNA as well as several proteins some of which could be involved in Acholeplasma-plant interactions [14, 16]. The same group also observed vesicles from Mycoplasma (M.) gallisepticum by atomic force microscopy but did not characterize them further [14].
Although they belong to the same Mollicutes class, bacteria from the genus Mycoplasma differ from those of the genus Acholeplasma. They are spherical, 0.3 to 1.0 μm in diameter [15] and carry a smaller genome (580–1350 kpb for mycoplasmas versus 1500–1650 kpb for acholeplasmas). Furthermore, unlike acholeplasmas, their membrane is rich in cholesterol that has to be provided by their growth environment as they are not able to synthesize it. Finally, whereas Acholeplasma species are most often regarded as opportunists, Mycoplasma species include several important pathogens for humans and animals. Hence, their capacity to produce EV might be of interest in terms of host-pathogen interactions.
The aim in the present work was to investigate EV release by several Mycoplasma species. A nutritional stress was applied to stimulate EV production and the general method recommended for EV purification was used and validated on the A. laidlawii model. Six Mycoplasma (sub)species, including pathogens of both human and animal origin, were shown to produce EV under nutritional stress. In vitro tests showed that EV are produced by living mycoplasma cells and are neither the result of dead cell lysis nor of aberrant cell division process. Proteomic analyses further revealed that EV-membranes contained proteins potentially involved in host-pathogen interactions.
Material and methods
Strains and culture conditions
The Acholeplasma and Mycoplasma species and strains used in this study are listed in Table 1. Of note for M. mycoides subsp. mycoides strain Afadé, only the TR-variant was used because i) it has no polysaccharide capsule, which is expected to facilitate EV release and ii) it expresses constitutively the glucose permease (MSC_0860) recognized by the 3f3 monoclonal antibody, which is used as a marker (see hereafter) [17]. They were propagated at 37°C under 5% CO2 in complete mycoplasma medium (PPLO) composed of a base (mycoplasma broth base 1.4% (w/v), tryptose 1.0% (w/v), yeast extract 0.3% (w/v), glucose 0.1% (w/v)), adjusted to pH 7.6, with addition of 30% supplement (horse serum 48% (v/v), pig serum 16% (v/v), fresh yeast extract 32% (v/v), cysteine 0.1% (w/v), NAD 0.1% (w/v), thallium acetate 0.3% (w/v)). For EV production the PPLO broth was modified (m-PPLO) by reducing the supplement fraction to 10% and adding 20% of 1X MEM α nucleoside (ThermoFisher) to the final medium to ensure substantial serum depletion (from 19% to 6%) without modifying the osmotic pressure. The supplement used for m-PPLO preparation was previously ultracentrifuged at 100 000g for 15h at 8°C in order to deplete potential exogenous eukaryotic extracellular vesicles. The PPLO and m-PPLO media were supplemented with amoxicillin 1g/l. Viable cell concentrations (cfu/ml) were determined by plating serial dilutions of liquid cultures onto PPLO agar plates. Each count was done in triplicate.
Follow-up and quality control of EV production.
M. mycoides subsp. mycoides strain Afadé variant TR was further used as a model to investigate the link between cell viability and EV production. Firstly, mycoplasma cells from a 24h-culture in m-PPLO medium (109 cfu/ml) were harvested (12000 g, 20 min, 18°C), resuspended in PBS and one half of the cells were incubated at 60°C for 1 hour while the other was incubated at room temperature for 1h. Cells from both batches were inoculated in m-PPLO medium and further incubated for 72h at 37°C before vesicles extraction and cell counts. In the second experiment, a 24h-culture (108 cfu/ml) was divided into two batches. One of the batches was supplemented with 200μg gentamicin/ml (a concentration known to be mycoplasmacidal [18]). A further 72h incubation at 37°C was performed before vesicles purification (see herafeter). The relative concentration of vesicles was estimated by electron microscopy and/or 3f3 immunobinding [19].
Isolation of extracellular vesicles
Acholeplasma and Mycoplasma strains were first cultivated in PPLO broth for 48h at 37°C, 5% CO2. Cells were harvested by centrifugation (12000g, 30min, 20°C), suspended in m-PPLO broth and further incubated at 37°C for 4 days, except for M. mycoides subsp. capri and M. capricolum subsp. capricolum, which were incubated for 2 days. Cells were removed by centrifugation at 14000g for 1h at 4°C and the supernatants were sterilized by filtering through 0.22 μm PVDF membranes. The filtrates were then concentrated 4-fold with Vivacell 70 MWCO 100 kDa (Sartorius). EV were collected after ultracentrifugation at 100 000g for 90 min at 8°C, then washed and suspended in 100 μl sterile PBS (10 mM phosphate, 150 mM NaCl, pH 7.8). All EV preparations were stored at -80°C and all further manipulations were carried out at 4°C. The absence of viable mycoplasma cells in EV preparations was ascertained by plating 25 μl (i.e. ¼) of the EV preparation onto PPLO agar plates.
Transmission electron microscopy (TEM) observation
The 200-mesh copper grids coated with Formvar-carbon were glow-discharged, and 5-μL samples were directly loaded onto the grids for two minutes before absorbing the liquid excess. The samples were then negatively stained by floating for 30 seconds on a drop of 1.0% (w/v) sodium silicotungstate. After air drying, images were acquired using a Philips CM120 TEM operated at 80 kV. EV diameter was determined using ImageJ software [20]. The mean EV density per (sub)species was estimated from the number of vesicles observed in ten 5 μm2 squares.
EV membrane proteomics
Since EV-protein quantification was biased by the presence of proteinaceous contaminants that co-purify with EV despite PBS washing (as observed in electron micrographs, see for example S2 Fig), EV-membrane proteins were extracted from 50μl of each EV preparation batch using Triton X-114 phase partitioning [21]. Proteins in the detergent phase were precipitated with methanol and chloroform, resuspended in Laemmli buffer and boiled for 5 min. Samples were electrophoresed on a miniprotean Any kd TGX gel (Bio-Rad) at 150 V for 5 min. The gels were stained with blue-safe staining from Bio-Rad according to the supplier’s instructions. Gel bands were excised and washed with DTT and iodoacetamide. In-gel tryptic digestion was performed overnight with 100 ng of trypsin (sequencing grade from Promega) in bicarbonate buffer 6h at 37°C. Peptides were extracted with 5% formic acid in water/acetonitrile (v/v), dried and suspended in 25μl of 0.1% formic acid (v/v) and 2% acetonitrile (v/v). LC MS/MS analyses were performed using an Ultimate 3000 RSLC system (Dionex) connected to a LTQ orbitrap mass spectrophotometer (ThermoFisher) by a nanoelectrospray ion source.
All MS/MS spectra were searched against Uniprot databases (Mycoplasma (M.) mycoides subsp. mycoides PG1T (Uniprot proteome identifier UP000001016, version 2013/10/11, 978 entries), M. agalactiae PG2T (Uniprot proteome identifier UP000007065, 11/04/2017, 726 entries) and M. fermentans PG18T (Uniprot proteome identifier UP000006810, 13/05/2017, 1091 entries) by the X!TandemPipeline (open source software developed by PAPPSO, version 3.4.3 [22]). The identified proteins were filtered using E-values <10−4 for proteins and <0.01 for peptides with a minimum of 2 peptides. A protein abundance index (PAI) was calculated for each protein in each sample using a relative quantification method, based on spectral counts. PAI, which reflects the relative abundance of the different proteins in each sample, is defined as the number of fragmentation spectra assigned with a significant score divided by the number of observable peptides per protein [23]. Membrane proteins, i.e. lipoproteins and transmembrane proteins were identified using Uniprot annotations and TMHMM2.0 prediction [24]. Other proteins were identified as either cytoplasmic or membrane-bound in reference to functional data but in the absence of characteristic structural features.
Results & discussion
Validation of our in-house experimental procedure for EV production
The nutritional stress applied to mycoplasma cultures involved growth in m-PPLO medium, which was partially-depleted in animal serum and fresh yeast extract to reduce the quantities of cholesterol, lipids, peptides, vitamins and nucleotides available for cell division. A. laidlawii strain PG8T was used as a control to validate our capacity to induce EV formation and perform purification. Cells were first cultivated in complete mycoplasma medium (PPLO) until the end of the log phase and then transferred to m-PPLO at a concentration of 108–109 cfu/ml for further incubation (Table 1). The titer of viable Acholeplasma cells remained steady for at least 24h and dropped to 107 cfu/ml at 96h (Table 1). EV were purified from the 96h-supernatant by ultracentrifugation and observed by TEM. The sizes ranged from 50 to 150 nm, with a few elements >150nm (Fig 1), consistent with the observations by Chernov and collaborators [14], and an estimated density of 5 EV/ 5μm2 field. The same experimental conditions were then tested on M. mycoides subsp. mycoides (Mmm) strain Afadé used as a representative of the Mycoplasma genus. Three different EV batches were prepared to assess the reproducibility of the technique. The viability of Mmm strain Afadé in m-PPLO was similar to that of A. laidlawii strain PG8T over time (Table 1). EV were observed for each production batch, with similar sizes ranging from 60 nm to 170 nm (with a few elements >170nm; Fig 1), and a density of around 30 EV/ 5 μm2 field (Table 1). Hence, our in-house experimental procedure confirmed the capacity of A. laidlawii PG8T to produce EV and demonstrated for the first time and in a reproducible manner the production of EV by Mmm strain Afadé.
EV diameters were estimated using Image J on n = 198 vesicles from A. laidlawii PG8T and n = 122, 129 and 149 vesicles from M. mycoides subsp. mycoides Afadé, corresponding to three production batches.
Because the diameter of the largest EV (from 170 to 220 nm in Fig 1) was very close to that of viable mycoplasma cells (from 300 to 1000 nm [15]) that could get smaller in nutritional stress conditions [25], the presence of viable cells in our EV preparations was checked by plating a quarter of each preparation on PPLO agar medium. No viable cell was detected in any production batch of Mmm, indicating that the largest EV are not small viable cells that could have been co-purified with EV, whereas 14 cells of A. laidlawii were found which corresponded to 56 cells in the whole batch (Table 1). Although this cell contamination was very limited (56 cells out of 1.8x1010 cfu in the whole culture after 96h incubation), it might affect the characterization of EV composition, notably regarding DNA/RNA content that relies on PCR amplifications. In consequence, we chose i) not to use a 0.1 μm filtering step that could potentially minimize cell contamination but might also retain some of the largest EV and ii) to systematically ascertain the quality of our EV preparation batches by performing a sterility control.
Microscopic observations of a Mmm Afadé culture in m-PPLO medium before EV purification showed a huge dispersion of spherical elements, including cells, and a clear overlapping area corresponding to EV (S1 Fig). Our EV isolation process resulted in a neat enrichment of the 60–170 nm EV and a depletion of the largest EV (170–220 nm, 3% in the EV preparation versus 13% in the Mmm culture; S1 Fig). Early microscopic observations showed membrane-surrounded vesicles (100–200 nm) named “elementary bodies” for several Mycoplasma species [26]. Such observations were confirmed by Robertson et al. on an aging culture of M. hominis in which small cell-like bodies (100–250 nm) associated in 0.22 μm-nonfilterable aggregates were evidenced [27]. Once dispersed by pronase treatment and transferred to favorable growth conditions these small cells turned out to be of spherical shape and viable, although poorly [27]. They were named at that time “elementary bodies”. Our EV isolation process involved a 0.22 μm filtration step and a viability control ensuring the depletion of such elementary bodies which suggests that the 3% largest structure in our EV preparation are really large EV and not elementary bodies resulting from aberrant cell divisions in unfavorable growth conditions.
Universality of EV production by Mycoplasma spp.
Our validated protocol was used to test the capacity of 5 other Mycoplasma (sub)species, belonging to two different phylogenetic groups, to produce EV (Table 1). To take into consideration the different loss of titer between fast growing, acidifying species (M. mycoides subsp. capri and M. capricolum subsp. capricolum) and others, EV were isolated from all species from supernatants obtained after either 48h or 96h (see Table 1). Fig 2 shows the spherical shape of EV isolated from different mycoplasma (sub)species. The mean respective diameters varied both between species and within species, as illustrated for M. agalactiae (Fig 3). The smallest vesicles were observed for M. agalactiae strain L14628 and M. bovis strain L15762. M. mycoides subsp. mycoides Afadé produced the largest EV. Similarly, the EV production yield, estimated by counting the mean number of EV per microscopic field varied considerably between species, M. fermentans strain PG18T and M. mycoides subsp. mycoides strain Afadé being the most productive under our experimental conditions (Table 1). Four out of seven EV preparations contained small amounts of viable cells (Table 1). This precluded any characterization of DNA/RNA content based on PCR techniques and further emphasized the difficulty of separating EV from minute sized cells characteristic of the Mycoplasma genus.
Examples of EV are indicated by black arrowheads.
Al, A. laidlaiwii PG8T; Mmm, M. mycoides subsp. mycoides Afadé; Mmc, M. mycoides subspp. capri PG3T; Mcc, M. capricolum subsp. capricolum L15937; Ma, M. agalactiae; Mb, M. bovis L15762; and Mf, M. fermentans PG18T. The number (n) of EV observed is indicated for each (sub)species. For Mmm, this “n” results from 3 batches of EV production.
Our m-PPLO medium inoculated with a high density of cells became suboptimal after 24h and viability started to decrease (loss of 1 to 3 log, Table 1). This raises the question of whether the observed EV might result from spontaneously reassembling membrane fragments of dead cells, i.e. could result from a degenerative process instead of being actively produced by viable cells. Two elements are in favor of an active EV production by viable cells. Firstly, the level of EV production is not related to cellular mortality in m-PPLO overtime but instead depends on species and strains: for instance, M. fermentans and M. bovis showed similar viable cell counts at 24h and 96h in m-PPLO although M. fermentans produced much more EV than M. bovis. Secondly, proteolipid vesicles artificially reconstituted from M. fermentans membranes were described as 1 μm-spheres [28], which is far larger than the EV observed here. This point was experimentally addressed by studying the EV production by heat- or gentamicin-killed Mmm strain Afadé cells. Mmm viability could be dramatically reduced by a 1h incubation at 60°C [29] or by treatment with 200 μg /ml gentamicin (i.e. 4-fold the MIC [30]). Indeed no viable cells were detected after heat treatment and a loss of 5 log was observed after 72h incubation with 200 μg/ml of gentamicin. EV production was quantified by immunodetection of the Mmm glucose permease (MSC_0860), a protein present in the membrane of Mmm EV (S1 Table) and specifically detected with high sensitivity by the 3f3 monoclonal antibody [19]. A correlation was indeed established between EV density estimated on electron micrographs and by the 3f3 detection by dot blotting (S2A Fig). Both heat and gentamicin treatment greatly reduced EV production (S2B Fig). This demonstrates that EV production relies on the presence of viable cells. Fig 4 further shows some putative vesicles budding from the cell surface of Mmm Afadé cells grown for 24h in m-PPLO medium. The size ratio between the cell and the vesicle is not characteristic of a binary fission and hence precludes the hypothesis of aberrant cell division.
A zoom of micrograph B is shown in the right panel. Diameters were estimated using imageJ.
Whatever the exact mechanism leading to EV release, it results in a multiplication of mycoplasma “forms/particles” that interact with the host cells. The protein content of EV-membranes was further analyzed to investigate its potential role in mycoplasma-host interactions.
Identification of virulence factors among the EV membrane associated proteins
The three EV preparations from Mycoplasma (sub)species showing none or negligible viable cell contamination (Table 1), i.e. M. mycoides subsp. mycoides Afadé, M. agalactiae 5632 and M. fermentans PG18T, were chosen to perform proteomic analyses on Triton X-114 enriched fractions. In these fractions 88, 58 and 258 proteins were identified, respectively, of which 54%, 88% and 54% were membrane-bound or membrane proteins (S1 Table). However, in our hands, the protein concentration in each Triton extract was not equivalent for the 3 species and hence the relative abundance of each protein was hardly comparable between species (S1 Table). A semi-quantitative scale of the PAI was established to compare which proteins were most abundant in each preparation (PAI ≥1.0 = ++++; [0.5–1.0 [= +++; [0.1–0.5 [= ++ and a spectral count <0.1 = + (S1 Table)).
In order to demonstrate that the produced vesicles could play a role in the pathogenesis process, we highlighted all EV-membrane associated proteins which could be involved in the mycoplasma-host interactions (Table 2).
Lipoproteins, which are known to be potent stimulators of macrophage activity associated with pro-inflammatory cytokines release [31], represented a non-negligible fraction of EV-proteins, ranging from 10 to 38%. As EV are able to disseminate a long distance from the infection site [32], the presence of lipoproteins in EV could contribute to the inflammatory process associated with mycoplasmoses. We further attempted to identify the EV-associated lipoproteins within each species that could play a role in interaction with the host (immune modulation, host colonization, interaction with host extracellular matrix…) (Table 2). A few of these lipoproteins were present in EV membrane fractions of all 3 species, including the p37 lipoprotein, which was shown to be oncogenic in M. fermentans [33]. Its action might be augmented as a result of dissemination through EV. Similarly the OppA lipoprotein that can induce apoptosis [34] is found in abundant proportions in both M. agalactiae and M. fermentans EV. Several other lipoproteins were identified, that are known to be major antigens of the different species, such as LppB and homologues [35]. These lipoproteins also exhibit several immunomodulatory properties, e.g. the production of IFNγ by Mmm LppA [36]. Variable surface proteins of M. agalactiae (Vpmas), which are involved in high frequency phase variation and hence immune escape, were also recovered from EV [37]. These Vpmas have recently been characterized as major adhesins [38]. M. agalactiae EV also carry a lipoprotein nuclease MAG5040 which has been proposed to allow neutrophil extracellular trap escape [39]. Hence several mycoplasma lipoproteins found in EV have functions related to modulation of the host immune response and to host colonization.
A similar pattern was detected for other membrane-bound proteins that are not lipoproteins. This was the case of the Elongation factor Thermo unstable (Ef-Tu) which was one of the most abundant proteins in each EV preparation. Interestingly, Ef-Tu was also found to be one of the most abundant proteins in Staphylococcus aureus EV [6]. This moonlighting protein was shown to interact with components of the host extracellular matrix [40, 41]. Its presence in each of the 3 batches of EV could argue in favor of EV release being a non-stochastic process although it could also reflect the fact that Ef-Tu is one of the most abundant bacterial proteins [41]. Similarly, the chaperone Hsp70 (DnaK) was found in the 3 EV-proteomes and was one of the most abundant proteins in Mmm strain Afadé and M. fermentans PG18T EV, based on spectral counts (Table 2 and S1 Table). Together with Ef-Tu, Hsp70 has been associated with antibody production, and cytokine secretion in M. ovipneumoniae [42]. Finally, Mmm Afadé and M. fermentans PG18T EV contained several enzymes of general metabolism such as lactate dehydrogenase, pyruvate dehydrogenase E1 enzyme, glyceraldehyde dehydrogenase, pyruvate kinase, phosphoglycerate kinase and transketolase, also known to interact with components of the host extracellular matrix [40]. The EV produced by Mmm Afadé were also enriched in the glucose permease MSC_0860, which had a practical interest as it was used as a marker for EV semi-quantification (see here before).
Mycoplasma proteins transported by vesicular structures had already been observed by electron microscopy as early as 1964 [43]. The authors described globular elements measuring 10 to 100 nm and carrying the then called “not-cell bound antigens”. Our analysis of EV membrane proteins confirmed that EV could be such carrier of antigens and could correspond to the globular structures described by Eng and Froholm [43]. Further identification of the complete cargo (soluble proteins including other antigens and DNA/RNA) has yet to be achieved but will require further improvement of the EV purification process, with a 100% efficient elimination of cell contaminations and protein aggregates. The use of gradient-based purification method might be a promising way [44].
Conclusions
Fifty years ago microscopic observations led to the conclusion that mycoplasma replicating cells had a minimal diameter of 300 nm. Vesicular structures such as “globular elements” (10–100 nm) and “elementary bodies” (100–250 nm) were also observed, the latter being considered the results of aberrant cell division or reassembling of membrane fragments. The concept of extracellular vesicles actively secreted by bacteria was just starting to emerge at that time and mainly for Gram negative. Here, we showed that EV can be released by several Mycoplasma species, from different phylogenetic clades, and are produced by living cells in a budding-way compatible with the canonical definition of bacterial EV. The sizes of mycoplasma EV vary considerably (from 30 to 220 nm) and setting a size cut-off between small viable cells and vesicles is difficult. Nonetheless the vesicles purified in this study are different from the elementary bodies described by Robertson as the latter are removed by 0.22 μm filtration [27]. The recurring presence of homologous proteins in EV-membranes preparations from 3 Mycoplasma species, further contributes to characterize EV release as an active process that could constitute a new “secretion” pathway and hence account for some of the proteins recovered in mycoplasma secretomes. For instance, the secretome from M. hyopneumoniae has several proteins in common with the EV-proteome described here [45]. Although it has to be formally demonstrated in the host context, the release of EV could considerably multiply mycoplasma interaction with the host cells. Mycoplasma EV as a potential component of the interactome will require further attention for a better understanding of mycoplasma pathogenicity and also for vaccine development.
Supporting information
S1 Fig. Comparison of size distribution of EV (n = 322, three production batches) purified from M. mycoides subsp. mycoides Afadé (black bars) and cells (n = 124) from a stationary phase culture of M. mycoides subsp. mycoides Afadé (white bars).
EV and cells were observed by TEM after negative staining and diameter was estimated using ImageJ.
https://doi.org/10.1371/journal.pone.0208160.s001
(TIF)
S2 Fig.
A. Validation of 3f3 dot blotting for EV semi-quantification. EV were extracted from 6h, 48h and 96h cultures of M. mycoides subsp. mycoides strain Afadé in m-PPLO medium. Three production batches were done for each time point. EV are indicated by black arrowheads on electron micrographs. Their density was estimated by counting the number of EV per 5 μm2 fields (scale: +/-, counts <1 EV/ 5μm2; +, 1–10 EV/ 5μm2; ++, 10–100 EV/ 5μm2). Dot blotting with 3f3 was performed on 2μl EV extract for each time point and each batch. The intensity of dot blotting correlates with the EV density in electron micrographs. B. Requirement of Mycoplasma viable cells for EV production. M. mycoides subsp. mycoides strain Afadé cultivated in m-PPLO medium (108–109 cfu/ml) was submitted to heat (1h at 60°C, no more viable cells) or chemical (200 μg/ml gentamicin, viability was reduced to 102 and 107 cfu/ml with or without gentamicin, respectively) inactivation before EV purification (for details see the Materials and methods section). EV (indicated by black arrowheads) density was estimated by counting on electron micrographs and/or by 3f3 dot-blotting (see panel A). When mycoplasma cells were killed no EV were produced.
https://doi.org/10.1371/journal.pone.0208160.s002
(TIF)
S1 Table. Proteins identified from the Triton X-114 fractions of EV.
Proteins are classified according to their PAI.
https://doi.org/10.1371/journal.pone.0208160.s003
(DOCX)
Acknowledgments
We thank Lucie Geay (UCBL, Lyon, France) for preparation of samples for TEM and Sandrine Magnard (IBCP, Lyon, France) for access to ultracentrifugation facilities. The authors declare no conflict of interest. S.G.’s PhD research is jointly funded by the French Agency for Food, Environmental and Occupational Health and Safety (Anses) and the French Agricultural Research Centre for International Development (CIRAD).
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