The vaginal microbiota, dominated by Lactobacillus spp., plays a key role in preventing HIV-1 transmission. Here, we investigate whether the anti-HIV effect of lactobacilli is mediated by extracellular vesicles (EVs) released by these bacteria. Human cervico-vaginal and tonsillar tissues ex vivo, and cell lines were infected with HIV-1 and treated with EVs released by lactobacilli isolated from vaginas of healthy women. EVs released by L. crispatus BC3 and L. gasseri BC12 protect tissues ex vivo and isolated cells from HIV-1 infection. This protection is associated with a decrease of viral attachment to target cells and viral entry due to diminished exposure of Env that mediates virus-cell interactions. Inhibition of HIV-1 infection is associated with the presence in EVs of several proteins and metabolites. Our findings demonstrate that the protective effect of Lactobacillus against HIV-1 is, in part, mediated by EVs released by these symbiotic bacteria. If confirmed in vivo, this finding may lead to new strategies to prevent male-to-female sexual HIV-1 transmission.
The vaginal microbiota, dominated mostly by Lactobacillus spp.1, plays a key role in defending the female genital tract against numerous urogenital pathogens, including HIV-12,3,4,5,6,7,8. In spite of the importance of this phenomenon, its mechanism remains largely unknown. Several mechanisms of Lactobacillus-mediated protection of vaginal cells from HIV-1 infection have been suggested by others2,9,10,11 and by us12. These include inactivation of HIV-1 through acidification of the vagina to pH∼4.5, capture of virions through bacterial membrane lectins, stimulation of anti-HIV-1 immune responses, and inhibition of the growth of pathogens responsible for bacterial vaginosis, which increase the risk of HIV-1 infection13.
Recently, it was found that Lactobacillus, along with other bacterial and mammalian cells, releases extracellular membrane vesicles. Extracellular vesicles (EVs) are implicated in cell–cell communications in various biological systems14,15,16. Cell–cell interactions in general, and microbiota–host-cell crosstalk in particular, are multifactorial phenomena that involve complex contact interactions between cells and cellular factors; many of these cellular factors such as lipids, proteins, nucleic acids, polysaccharides, and various soluble factors are associated with EVs. Noticeably, until the last decade it was believed that Gram-positive bacteria were not capable of releasing EVs because of their thick cell walls. However, Lee et al.17 showed that Staphylococcus aureus releases EVs17. In subsequent studies, EVs have been also isolated from Lactobacillus strains18,19,20,21,22,23,24.
Although the role of Gram-positive bacterial EVs has been less studied than that of mammalian EVs or even Gram-negative bacteria, it was found that Gram-positive-derived EVs from Lactobacillus can stimulate the host immune and nervous systems18, enhance the host immune responses against other bacteria24, and induce cell apoptosis in hepatic cancer cells19.
We hypothesized that EVs released by lactobacilli contribute to the Lactobacillus-mediated protection of vaginal viral infection. This protection can be simulated ex vivo, as we demonstrated earlier: several strains of vaginal Lactobacillus inhibited HIV-1 infection in human cervico-vaginal and tonsillar tissues ex vivo12. Human tissues ex vivo retain tissue cytoarchitecture and provide an adequate experimental model to study the pathogenesis of various human viruses25, in particular HIV-1.
Here, we investigate whether EVs derived from four different strains of Lactobacillus (L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, and L. gasseri BC13) isolated from vaginas of healthy women6 are capable of inhibiting HIV-1 infection. The choice of these Lactobacillus strains is based on the earlier reported anti-HIV-1 activity of these bacteria in human tissues ex vivo12. Moreover, these bacterial strains are the ones that mostly dominate the vaginal ecosystem1. We demonstrate that EVs released by lactobacilli into culture medium protect human T cells as well as human cervico-vaginal and tonsillar tissues ex vivo from HIV-1 infection. This protection is mediated, in part, by inhibition of viral attachment and entry to target cells due to diminished exposure of Env on EV-treated HIV-1 virions. Furthermore, using proteomic and metabolomic analysis, we identify several EV-associated bacterial proteins and metabolites that may play a role in this protective effect against HIV-1 infection.
Lactobacilli EVs in HIV-1 inhibition
Here, we characterized the EVs released by symbiotic vaginal lactobacilli in terms of their size and concentration, tested their anti-HIV-1 effect in human T cells and tissues, evaluated EV cytotoxicity, and identified EV-associated bioactive molecules that may contribute to the anti-HIV-1 inhibitory activity of the EVs studied.
Characterization of EVs released by Lactobacillus
We used NTA to characterize the sizes and concentrations of bacterial EVs produced by L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, and L. gasseri BC13. We isolated EVs by ultracentrifugation from bacteria cultures (50 mL, 1 × 109 CFU per mL). All the tested bacteria released EVs of similar size, with mean diameters ranging from 133.14 ± 2.90 nm (L. crispatus BC3) to 141.26 ± 9.78 nm (L. crispatus BC5) (Fig. 1a, b). The concentration of EVs released varied from one bacterial strain to another: 3.26 ± 0.11 × 1010 (L. crispatus BC3), 1.18 ± 0.32 × 1010 (L. crispatus BC5), 5.87 ± 0.20 × 1010 (L. gasseri BC12), and 1.32 ± 0.44 × 1011 (L. gasseri BC13) particles per mL (Fig. 1c). Although MRS medium not conditioned by bacteria also contained particles, their concentrations were about two orders of magnitude lower (4.13 ± 0.70 × 109 particles per mL) than those of EVs released by bacteria (Fig. 1c). However, no specific protein bands were found in MRS-isolated particles in contrast to bacterial EVs. Moreover, we did not find eukaryotic EV markers (TSG101, CD63) in any Lactobacillus-derived EVs tested in our study compared with the positive control (MT-4 cell lysates), demonstrating that the preparation of bacteria-derived EVs did not contain eukaryotic EVs (Fig. 1d).
The average size of these particles was statistically not different from that of bacteria-derived EVs (162 ± 4.27 nm) (Fig. 1a, b).
Bacterial EVs suppress HIV-1 infection in human cell lines
To investigate whether Lactobacillus-derived EVs affect HIV-1 infection, we infected two human CD4+ T cell lines, MT-4 and Jurkat-tat, with this virus. We worked with a prototypic HIV-1 that uses CD4 and CCR5 cell-surface coreceptor to enter cells and is typical at the early stages of infection (isolate BaL) and a prototypic HIV-1 that uses CD4 and CXCR4 cell-surface coreceptor that often evolves at the late stages of infection (isolate LAI.04). Levels of HIV-1 infection were monitored from measurements of the release of HIV-1 gag protein p24 into the culture medium.
HIV-1LAI.04 infection of MT-4 cell cultures varied from 3.75 × 104 to 1.29 × 107 p24gag pg per mL. As shown in Fig. 2a, HIV-1LAI.04 replication in MT-4 cells was reduced by 91.88 ± 3.15% (p < 0.0001, n = 14, repeated-measures analysis of variance (ANOVA)) when cells were treated with L. gasseri BC12-derived EVs (5 × 108 particles per mL) and by 59.35 ± 2.34% (p < 0.0001, n = 5, repeated-measures ANOVA) when MT-4 cells were treated with L. crispatus BC3-derived EVs. In contrast, no statistically significant HIV-1LAI.04 inhibition was observed when MT-4 cell cultures were treated with similar numbers of EVs from L. crispatus BC5 (p = 0.9967, n = 7, repeated-measures ANOVA) or L. gasseri BC13-derived EVs (p = 0.8750, n = 4, repeated-measures ANOVA). Also, there was no inhibition of HIV-1 replication in MT-4 cells treated with particles isolated from MRS medium (p = 0.9706, n = 4, repeated-measures ANOVA) (Fig. 2a).
We chose EVs released from L. gasseri BC12, which showed a higher capacity to inhibit HIV-1 replication than the other bacterial-derived EVs, as a model condition to test the concentration-dependent anti-HIV-1 effect. Inhibition of HIV-1LAI.04 infection of MT-4 cells by EVs was concentration dependent: L. gasseri BC12-derived EVs at a concentration of 5 × 104 EVs per mL suppressed HIV-1LAI.04 replication by 14.59 ± 3.23% (p = 0.04232, n = 15, repeated-measures ANOVA), and the effect progressively augmented with increase in the concentration of bacterial EVs, reaching an inhibition of viral replication by 93.48 ± 0.69% (p < 0.0001, n = 15, repeated-measures ANOVA) at a concentration of 5 × 108 EVs per mL (Fig. 2b).
The inhibition of HIV-1BaL infectivity in Jurkat-tat cells by L. gasseri BC12-derived EVs was also concentration dependent: EVs at a concentration of 5 × 104 EVs per mL inhibited HIV-1BaL replication by 33.18 ± 9.16% (p = 0.0007, n = 8, repeated-measures ANOVA), whereas EVs at 5 × 108 EVs per mL inhibited viral replication by 98.71 ± 0.56% (p < 0.0001, n = 10, repeated-measures ANOVA) (Fig. 2c). At the highest concentration of EVs, 5 × 108 EVs were added to 5 × 105 cells, and therefore the ratio was ~1000 EVs per cell.
Treatment of HIV-1-infected MT-4 cells with bacterial EVs did not affect the expression of p53 level, typically elevated after HIV-1 infections26,27,28 (Supplementary Fig. 1).
Bacterial EVs are not cytotoxic
To check whether EV treatment decreases the viability of EV-treated cells, we evaluated the possible cytotoxic effect of EVs secreted by four Lactobacillus strains (L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, L. gasseri BC13) on MT-4 and Jurkat-tat cell lines. Toward this goal, human T cells were cultured in a medium containing or not containing 5 × 108 bacterial EVs per mL. We also tested the particles isolated from bacteria-free MRS medium (5 × 108 particles per mL) in an experimental control condition. We used Triton X-100 at 0.2% as a positive control in the toxicicty assays. After 3 days of cell treatment, we evaluated cell viability from counts of the total and dead cells in control and EV-treated cultures using a propidium-iodide-based assay. There was no decrease in the number of viable cells after treatment with different amounts of Lactobacillus-derived EVs or similarly isolated particles from MRS medium in comparison with untreated controls, both in MT-4 and in Jurkat-tat cell cultures (Fig. 3a). The viability of cells treated with the highest amount of bacterial EVs (5 × 108 EVs per mL) was statistically not different (p > 0.13, repeated-measures ANOVA) from that in untreated controls (100%), ranging from 88.90 ± 2.54% (L. crispatus BC13-derived EVs) to 113.20 ± 6.57% (L. crispatus BC3-derived EVs) in MT-4 cells and from 90.95 ± 1.68% (L. crispatus BC13-derived EVs) to 102.80 ± 3.52% (L. crispatus BC3-derived EVs) in Jurkat-tat cells. Similarly, the cell viability upon treatment with MRS medium-derived particles was not altered compared with the control (p > 0.39, repeated-measures ANOVA) in both cell lines (89.91 ± 4.70% and 90.86 ± 3.85% in MT-4 and Jurkat-tat, respectively). On the other hand, as expected, Triton X-100 at 0.2% reduced the cell viability significantly, down to 7.81 ± 0.53% (p < 0.0001, repeated-measures ANOVA) in MT-4 cells and 8.66 ± 0.30% (p < 0.0001, repeated-measures ANOVA) in Jurkat-tat cells.
Similar results were obtained with the MTT assay (Fig. 3b). Indeed, the percentages of viable cells were not altered significantly (p > 0.17, repeated-measures ANOVA) by particles from MRS medium or by bacterial EVs compared with the control. The cell viability in MT-4 cells ranged from 99.20 ± 3.59% (L. crispatus BC3-derived EVs) to 116.70 ± 2.56% (MRS-derived particles) for MT-4 cells and from 97.16 ± 1.90% (L. crispatus BC5-derived EVs) to 105.00 ± 1.83% (L. crispatus BC13-derived EVs) for Jurkat-tat cells. Instead, treatment with Triton X-100 at 0.2% reduced the cell viability significantly, down to 27.91 ± 2.61% (p < 0.0001, repeated-measures ANOVA) in MT-4 cells and by 15.46 ± 0.31% (p < 0.0001, repeated-measures ANOVA) in Jurkat-tat cells.
The lack of EV cytotoxicity was confirmed by flow cytometry. EV-treated and control cell cultures were stained with live/dead Fixable Viability Dye, anti-CD3-, and anti-CD4-antibodies, and were then enumerated with a flow cytometer. There was no significant difference between fractions of live, CD3+, and CD4+ MT-4 cells 3 days post L. gasseri BC12-derived EV treatment (5 × 108 EVs per mL; CD3+ cells: 99.91%, CD4+ cells: 98.54%) and respective control values (CD3+ cells: 99.80%, CD4+ cells: 99.54%) (Fig. 3c, Supplementary Fig. 2).
Bacterial EVs suppress HIV-1 infection in human tissues
We investigated whether Lactobacillus-derived EVs can suppress HIV-1 infection in human tonsillar and cervico-vaginal tissues ex vivo. Human tonsillar tissues ex vivo infected with HIV-1BaL were cultured in medium containing or not containing equal amounts of EVs (5 × 108 EVs per mL) isolated from culture media derived from four Lactobacillus strains: L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, L. gasseri BC13, and MRS medium-derived particles. As shown in Fig. 4a, HIV-1BaL replication was significantly reduced, by 38.70 ± 11.36% (p = 0.0199, n = 5, repeated-measures ANOVA), when tonsillar tissue blocks were cultured in presence of EVs derived from L. crispatus BC3, and by 48.19 ± 10.11% (p = 0.0033, n = 5, repeated-measures ANOVA) when cultured in presence of EVs derived from L. gasseri BC12, compared with tonsillar tissue blocks cultured in the absence of bacterial EVs.
There was no statistically significant inhibition of HIV-1BaL replication in tonsillar tissues cultured ex vivo in the presence of EVs derived from L. crispatus BC5 (p = 0.4602, n = 5, repeated-measures ANOVA) or L. gasseri BC13 (p = 0.4744, n = 5), or particles derived from MRS medium (p > 0.9999, n = 4, repeated-measures ANOVA).
In ex vivo tissues, we also evaluated the concentration dependency of HIV-1 suppression by bacterial EVs. We cultured tonsillar tissue blocks infected with HIV-1LAI.04 and cervico-vaginal tissue blocks infected with HIV-1BaL in the presence of tenfold serial dilutions of EVs derived from L. gasseri BC12 (5 × 105; 5 × 106, 5 × 107, 5 × 108 EVs per mL). The inhibitory effect of L. gasseri BC12-derived EVs on HIV-1LAI.04 replication in tonsillar tissue blocks was concentration dependent, with a 20.92 ± 7.54% inhibition (p = 0.0236, n = 5, repeated-measures ANOVA) with EVs at a concentration of 5 × 106 EVs per mL and a 61.03 ± 5.58% (p < 0.0001, n = 5, repeated-measures ANOVA) inhibition at the maximal tested EV concentration (5 × 108 EVs per mL) (Fig. 4b). A similar concentration dependency of bacterial EVs on HIV-1 replication was obtained in cervico-vaginal tissues, where HIV-1BaL replication was inhibited by 31.30 ± 3.22% (p = 0.028, n = 4, repeated-measures ANOVA) when EVs were present at 5 × 105 EVs per mL and by 59.83 ± 4.92% (p < 0.0001, n = 4, repeated-measures ANOVA) when EVs were present at 5 × 108 EVs per mL (Fig. 4c). In the above-described experiments with tonsillar tissue explants, nine tissue blocks were cultured in 3 mL of medium. Therefore, 1.5 × 109 EVs were used (5 × 108 EVs per mL × 3) for a total of ~1.08 × 106 CD4 + T cells (~1.2 × 105 CD4 + T cells per block × 9 blocks)25, thus giving a ratio of 1000 EVs per cell.
Bacterial EVs reduce HIV-1 entry/attachment to target cells
To investigate whether the inhibition of HIV-1 replication was associated with a decrease in viral entry, we used TZM-bl cells. HIV-1 infection of these cells was reduced in a concentration-dependent manner. Luciferase expression was decreased by 38.52 ± 8.74% (p = 0.001, n = 6, repeated-measures ANOVA) when HIV-1LAI.04-infected TZM-bl cells were incubated with EVs from L. gasseri BC12 at a concentration of 5 × 106 EVs per mL and by 69.45 ± 6.10% (p < 0.0001, n = 6, repeated-measures ANOVA) at a concentration of 5 × 108 EVs per mL. In contrast, no statistically significant HIV-1LAI.04 entry inhibition was observed when TZM-bl cell cultures were treated with particles from MRS (p = 0.9661, n = 3, repeated-measures ANOVA) at 5 × 108 EVs per mL (Fig. 5a).
The effect of Lactobacillus EVs on HIV-1 attachment/entry was also studied in MT-4 cell line. MT-4 cells were incubated with HIV-1LAI.04 for 2 h at 4 °C, in the presence or absence of EVs derived from L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, or L. gasseri BC13, or of particles derived from MRS medium. After eliminating all free viral particles with several washes, we observed that the levels of HIV-1 p24gag, were reduced significantly upon the incubation with EVs derived from L. crispatus BC3, by 63.31 ± 4.74% (p < 0.0001, n = 3, repeated-measures ANOVA), and with EVs derived from L. gasseri BC12, by 80.41 ± 5.35% (p < 0.0001, n = 6, repeated-measures ANOVA) (Fig. 5b). In contrast, there was no statistically significant reduction of p24gag levels when virions were treated with EVs derived from L. crispatus BC5 (p = 0.0517, n = 3, repeated-measures ANOVA), with L. gasseri BC13-derived EVs (p = 0.9276, n = 3), or with particles derived from MRS medium (p = 0.9999, n = 3, repeated-measures ANOVA).
Bacterial EVs prevent HIV-1 infection affecting viral Env
To investigate whether Lactobacillus-derived EVs affect HIV-1 envelope directly, we pretreated HIV-1LAI.04 virions with EVs derived from four Lactobacillus strains (L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, and L. gasseri BC13) for 1 h. Then, we captured HIV-1LAI.04 virions using PG9 antibodies coupled to magnetic nanoparticles (MNPs). PG9 preferentially recognizes the HIV-1 trimeric envelope proteins (gp120). As shown in Fig. 6, the amounts of HIV-1LAI.04 viral particles captured, as measured from HIV-1 p24gag concentration, were reduced significantly, by 59.93 ± 4.55% (p < 0.0001, n = 3, repeated-measures ANOVA) upon viral pretreatment with EVs derived from L. crispatus BC3 and by 64.32 ± 2.78% (p < 0.0001, n = 3, repeated-measures ANOVA) when HIV-1LAI.04 were pretreated with EVs derived from L. gasseri BC12, compared with the captured viral particles in the absence of bacterial EVs.
There was no statistically significant effect on the HIV-1LAI.04 envelope when virions were pretreated with EVs derived from L. crispatus BC5 (p = 0.6590, n = 3, repeated-measures ANOVA) or L. gasseri BC13-derived EVs (p = 0.5654, n = 3, repeated-measures ANOVA), or with particles derived from MRS medium (p = 0.9011, n = 3, repeated-measures ANOVA).
EV treatment of cells does not prevent HIV-1 infection
To study whether bacterial EVs alter host cell function to induce protection against HIV-1, TZM-bl, or MT-4 cells were cultured in cell culture medium containing or not containing bacterial EVs for 24 h, prior to HIV-1 infection, and HIV-1 infection was evaluated. As shown in Fig. 7a, HIV-1LAI.04 replication was not significantly reduced upon pretreatment with bacterial EVs derived from L. crispatus BC3 (p = 0.3665, n = 4, repeated-measures ANOVA), L. crispatus BC5 (p = 0.0972, n = 4, repeated-measures ANOVA), L. gasseri BC12 (p = 0.2031, n = 4, repeated-measures ANOVA), L. gasseri BC13 (p = 0.0594, n = 4, repeated-measures ANOVA) or upon pretreatment with MRS-derived particles (p = 0.0515, n = 4, repeated-measures ANOVA), compared with control experiments.
Similar results were obtained in MT-4 cells. HIV-1LAI.04 replication was not significantly reduced upon pretreatment with bacterial EVs derived from L. crispatus BC3 (p = 0.31901, n = 3, repeated-measures ANOVA), L. crispatus BC5 (p = 0.1286, n = 3, repeated-measures ANOVA), L. gasseri BC12 (p = 0.8680, n = 3, repeated-measures ANOVA), L. gasseri BC13 (p = 0.1127, n = 3, repeated-measures ANOVA) or upon pretreatment with MRS-derived particles (p = 0.7353, n = 3, repeated-measures ANOVA) (Fig. 7b).
Metabolites associated with Lactobacillus-derived EVs
We used 1H-NMR to identify metabolites that are associated with bacterial EVs. The metabolomic analysis was conducted on EVs derived from Lactobacillus strains that inhibited HIV-1 replication (L. crispatus BC3, L. gasseri BC12), on EVs that did not inhibit HIV-1 replication (L. crispatus BC5, L. gasseri BC13), and as well on particles isolated from MRS medium. To release all the EV content, we sonicated them prior to the analysis. We identified 42 molecules, mainly belonging to the classes of organic acids, amino acids, sugars, and nitrogen bases (Supplementary Table 1). Five of them were found to correlate significantly with the antiviral activity. To highlight their underlying trends, these molecules were employed as a basis for an rPCA model (Fig. 8a). Two principal components (PC) appeared to describe the variance of the samples optimally. PC 1, accounting for 74.8% of the variance described by the model, accounted for the sample’s antiviral activity against HIV-1. EVs derived from L. crispatus BC3 and L. gasseri BC12, which efficiently suppress HIV-1 inhibition, showed lower PC 1 scores. EVs from L. crispatus BC5 and L. gasseri BC13, which did not inhibit HIV-1, showed higher PC 1 scores. L. crispatus BC3- and L. gasseri BC12-derived EVs were mainly associated with high amounts of methionine, glycine, hypoxanthine, and glutamate. In contrast, EVs derived from L. crispatus BC5 and L. gasseri BC13, as well as particles derived from MRS medium, were mainly characterized by the presence of asparagine (Fig. 8b).
The samples from the same bacterial strains showed similar PC scores, thus suggesting a good biological reproducibility of the metabolome’s profile.
Proteins associated with Lactobacillus-derived EVs
We then investigated which proteins of Lactobacillus-associated EVs could be responsible for the above-described HIV-1 suppression by L. gasseri BC12 in comparison with EVs released by L. crispatus BC5, which do not suppress HIV-1 infection.
Using liquid chromatography–mass spectroscopy, we investigated the spectra of bacterial proteins present in the EVs of L. gasseri BC12 and L. crispatus BC5. Altogether, we identified 18 bacterial proteins associated with EVs derived from these two Lactobacillus strains (Table 1, Supplementary Table 2). Fifteen proteins were identified in EVs derived from L. gasseri BC12 and eleven proteins were identified in EVs released by L. crispatus BC5. Seven proteins were found in both L. gasseri BC12- and L. crispatus BC5-derived EVs. These were ATP synthase subunit beta from L. gasseri, ATP synthase subunit alpha, phosphonates import ATP-binding protein PhnC, ATP synthase subunit b, enolase 1, ATP synthase subunit beta, and 30S ribosomal protein S4. Eight proteins (enolase 2, 60 kDa chaperonin, elongation factor Tu, ATP synthase gamma chain, foldase protein PrsA 1, ATP synthase subunit delta, pyruvate kinase, and triosephosphate isomerase) were identified only in EVs derived from L. gasseri BC12, and three proteins (50S ribosomal protein L4, 50S ribosomal protein L21, and 50S ribosomal protein L2) were identified only in EVs derived from L. crispatus BC5.
According to the protein localization in the cellular component by Gene Ontology (GO) terms (Fig. 9a, Supplementary Table 2), the majority of the identified proteins associated either with L. gasseri BC12- or L. crispatus BC5-derived EVs were in the cytoplasm (44.44%, 45.45%) and membrane (44.44%, 45.45%), respectively. The remainder of the proteins exert their activities extracellularly (11.11%, 9.09%).
According to the molecular functions by the GO terms (Fig. 9b, Supplementary Table 2), most of the EV-related proteins identified in both L. gasseri BC12- and L. crispatus BC5-derived EVs are involved in ATP binding (20.00%, 20.00%), proton-transporting ATP synthase activity (15.00%, 20.00%), rotational mechanism (15.00%, 20.00%), magnesium ion binding (10.00%, 5.00%), phosphopyruvate hydratase activity (5.00%, 5.00%), rRNA binding (2.50%, 20.00%), and ATPase-coupled organic phosphonate transmembrane transporter activity (2.50%, 5.00%), respectively. The proteins associated with EVs derived from L. gasseri BC12 are also involved in kinase activity (5.00%), potassium ion binding (5.00%), pyruvate kinase activity (5.00%), unfolded protein binding (2.50%), GTP binding (2.50%), GTPase activity (2.50%), translation elongation factor activity (2.50%), peptidyl-prolyl cis–trans isomerase activity (2.50%), and triosephosphate isomerase activity (2.50%). The proteins identified in EVs from L. crispatus BC5 only, are also involved in transferase activity (5.00%).
Mammalian mucosae are populated by numerous bacteria that collectively form the microbiota that controls many of the host’s normal and pathological processes. In particular, a vaginal microbiota dominated by Lactobacillus species is protective against various pathogens, including HIV-11,2,13.
Microbiota–host-cell crosstalk is a complex multifactorial phenomenon. A growing body of evidence suggests that one of the important mediators of cell–cell communications is nanosized extracellular vesicles (EVs), produced by all domains of life, including archaea, fungi, parasites, and bacteria14,29,30. Initially, it was thought that, in contrast to Gram-negative bacteria, Gram-positive bacteria including Lactobacillus could not produce EVs because of their thick cell walls. However, it was shown recently that Gram-positive bacteria are capable of releasing phospholipid bilayer nanosized EVs with a diameter range from 20 to 200 nm, like Gram-negative- or eukaryotic-derived EVs15,17,20.
Here, we report for the first time on the production of EVs by Lactobacillus strains of human vaginal origin. We demonstrated that vaginal lactobacilli (L. crispatus, L. gasseri) release nanosized EVs similar to those released by Lactobacillus strains of gastrointestinal origin such as L. casei, L. rhamnosus, L. reuteri, and L. plantarum18,19,21,22,23,24. Preparation of EVs isolated from lactobacilli cultured in MRS medium did not contain eukaryotic EV markers. Also, no specific protein bands were found in MRS-isolated particles in contrast with bacterial EVs. This may be expected since the MRS medium was autoclaved, which most likely resulted in denaturation of the proteins present in the MRS medium. Nevertheless we included these particles as experimental control conditions.
We investigated whether EVs released by lactobacilli contribute to the protective effect of Lactobacillus against vaginal HIV-1 infection2,9,10,11. We addressed this question by using immortalized human T cells as well as human cervico-vaginal tissue and lymphoid tonsillar tissues ex vivo. The ex vivo model is the standard tissue culture for study of HIV-1 pathogenesis, as it faithfully reflects many aspects of tissues where critical events in HIV-1 transmission and pathogenesis occur in vivo. Tissues ex vivo support productive HIV-1 infection without exogenous activation or stimulation and retain the pattern of expression of key cell-surface molecules relevant to HIV-1 infection25. Also, in a previous study, we demonstrated that various strains of Lactobacillus isolated from vaginas of healthy individuals inhibit HIV-1 replication in human cervico-vaginal and tonsillar tissues ex vivo12. Specifically, we found that L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, and L. gasseri BC13 largely protected human ex vivo tissues from HIV-1 infection.
Here, we showed that this protection can be mediated by bacterial EVs. EVs released by L. crispatus BC3 and L. gasseri BC12 largely protected human tissues ex vivo and T cells from HIV-1 infection. The HIV-1 inhibitory effects of EVs from L. crispatus BC3 or L. gasseri BC12 were dose-dependent. At the highest concentration used in our study there were ~1000 EVs per HIV-1 target cell. At this concentration, EVs were not cytotoxic, as evaluated with three different techniques (propidium-iodide-based assay, flow cytometry, and MTT assay). Thus, inhibition of HIV-1 infection was not due to EV-induced cell death.
Not all lactobacilli-released EVs inhibited HIV-1 infection: EVs from L. crispatus BC5 or L. gasseri BC13 did not inhibit HIV-1 infection, although these bacterial strains inhibited HIV-1 replication in human tissues ex vivo12. The difference in behavior between EVs released by L. crispatus BC3 and L. gasseri BC12 and between L. crispatus BC5 and L. gasseri BC13 could in principle be due to the different quantity of EVs released by these bacteria or to their qualitative features. We found that there was no difference in either the number or the size distribution between EVs that inhibited and those that did not inhibit HIV-1 infection. Thus, the inhibitory activity of EVs from L. crispatus BC3 and L. gasseri BC12 is not quantitative but rather is related to their composition.
We identified differences in composition between HIV-1-inhibiting and HIV-1-noninhibiting EVs through proteomic and metabolomic analysis. First, the difference in metabolite composition between EVs that inhibit and those that do not inhibit HIV-1 infection was revealed by the principal component analysis of metabolomics: high anti-HIV-1 activity of EVs correlated with their metabolomic profiles. In particular, EVs active toward HIV-1 infection were mainly associated with high amounts of amino acids. Also, our data demonstrated the presence of lactic acid in association with EVs released by lactobacilli. Lactic acid is a metabolite known to exert an anti-HIV-1 effect4,12,31,32. The use of lactic-acid-containing diaphragm gel to suppress HIV-1 recently passed Safety Phase I in a pre-clinical study33.
Proteomic analysis also showed that EVs that inhibited HIV-1 replication differ from those that did not inhibit the virus in terms of several proteins, namely enolase 2, 60 kDa chaperonin, elongation factor Tu, ATP synthase gamma chain, foldase protein PrsA 1, ATP synthase subunit delta, and triosephosphate isomerase. Similar proteins were identified in EVs released by the gastrointestinal bacterium, Lactobacillus casei22.
Bioactivity of several molecules that we identified in HIV-1-inhibiting EVs was reported earlier: several enolases derived from Lactobacillus were shown to inhibit the adherence of Neisseria gonorrhoeae to epithelial cells34. Moreover, bifidobacterial enolase, a cell-surface receptor for human plasminogen, was involved in interaction with human host cells35. The elongation factor Tu was shown to play an important role in the attachment of Lactobacillus johnsonii to human intestinal cells and mucins36. Whether the inhibition of HIV-1 entry is the result of the action of one or of a combination of several of these bioactive molecules acting synergically remains an open and somewhat difficult question to answer. Also, they may act only when associated with EVs. For these reasons, we tested the effect of EVs as a whole in a cellular model of HIV-1 entry using TZM-bl cells. TZM-bl cells contain integrated reporter genes for firefly luciferase and E. coli β-galactosidase under the control of an HIV-1 long terminal repeat37,38, permitting sensitive and accurate measurements of infection at the entry/attachment level. Here, we showed that viral attachment/entry to TZM-bl cells was inversely proportional to the concentration of bacterial EVs. Another set of experiments performed in the T cell line MT-4 confirmed that EVs directly inhibit HIV-1 attachment to cells. Thus, the anti-HIV-1 effect of Lactobacillus-derived EVs is mediated by the decrease of viral entry/attachment to the target cells.
This decrease may be related to the alteration of HIV-1 virions by bacterial EVs. We found that virions pretreated with EVs released by L. crispatus BC3 and L. gasseri BC12, but not by L. crispatus BC5 and L. gasseri BC13, were no longer recognized by PG9, an antibody that specifically binds functional trimeric gp120. Bacterial EVs from L. crispatus BC3 and L. gasseri BC12 interfere with the acessability of viral Env, thus explaining HIV-1 inhibition observed in cell lines and in human tissues ex vivo. In contrast, the pretreatment of cells with bacterial EVs did not affect HIV-1 infection. Bacterial EV-mediated HIV-1 inhibition is therefore the consequence of EVs affecting the infectivity of virions rather than cell functions.
Also, there could be other mechanisms by which EVs inhibit HIV-1 infection. Gram-positive bacteria-derived EVs can change susceptibility of cells to viral infection, e.g., by regulating TLR2 activity39, by delivering signal molecules into the cells40,41,42, or by upregulating host defense genes24.
Also, bacterial EVs may prevent HIV-1 infection by affecting the vaginal mucosa immune activation status. It has already been demonstrated that the vaginal microbiota, in particular Lactobacillus species, affects the immune system in such a way as to efficiently prevent viral infections13,43,44,45. Whether these immunomodulatory effects may be mediated by EVs released from Lactobacillus remains to be studied.
In conclusion, in our ex vivo tissue system the protective effect of vaginal Lactobacillus against HIV-1 transmission is, in part, mediated by bacterial EVs that inhibit HIV-1 attachment/entry to the target cells due to diminished exposure of viral Env. To extrapolate our findings to the in vivo context, direct experiments in in vivo systems should be performed. These findings may lead to new strategies to prevent male-to-female sexual HIV-1 transmission, for example by use of EVs derived from symbiotic bacteria.
Bacterial cultures and extracellular vesicle isolation
All Lactobacillus strains of vaginal origin, L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, and L. gasseri BC136, were cultured overnight at 37 °C in tubes containing 50 mL of de Man, Rogosa, and Sharpe (MRS) broth (Difco, Detroit, MI) supplemented with 0.05% L-cysteine. MRS broth was previously autoclaved and filtered with 0.1-μm filters to reduce the amount of particles that might be present in the medium. We achieved anaerobic conditions by cultivating lactobacilli in jars containing Gaspak EZ (BD, Franklin Lakes, NJ). We measured the turbidity of overnight cultures with a spectrophotometer (OD600 nm; Biophotometer, Eppendorf, Germany) and calculated the bacterial concentration using an optical density conversion factor of 0.4, corresponding to a concentration of 108 colony-forming units (CFU) per mL. EVs were isolated by sequencial ultracentrifugation46. 50 mL of bacterial suspension (1 × 109 CFU per mL) was centrifuged at 2500 × g for 10 min at 4 °C. The resulting supernatants were filtered with 0.22-μm filters to eliminate any remaining bacteria. We obtained EVs by ultracentrifuging the samples at 100,000 × g for 70 min at 4 °C (Ultracentrifuge WX ultra 80, Rotor: AH629 capacity 6 × 36 mL; Thermo Fisher Scientific, Walkersville, MD). The pellet containing bacterial EVs was washed in phosphate-buffered saline (PBS), ultracentrifuged (as specified above), and resuspended in 150 μL of PBS and stored at 4 °C. The same protocol was applied to isolate particles from 50 mL of MRS medium.
Nanoparticle tracking analysis of bacterial EVs
Nanoparticle tracking analysis (NTA) utilizes the properties of both light scattering and Brownian motion to obtain the particle size distribution of samples in liquid suspension. Briefly, we diluted EVs 1:100 in PBS and tracked them using the NanoSight NS300 (Malvern instruments Ltd, Malvern, UK) equipped with a 405-nm laser. The samples were flowed by means of a constant pressure syringe pump controller. Videos were recorded for 60 s three times, at camera level 13, and analyzed with NTA software 3.0 (Malvern instruments Ltd, Malvern, UK).
Cell and human tissue cultures
Human T-lymphocyte MT-4 (obtained through the NIH AIDS Reagent Program, Germatown, MD, catalog number 120) and Jurkat-tat cell lines (obtained through the NIH AIDS Reagent Program, Germatown, MD, catalog number 1399) were cultured in Roswell Park Memorial Institute (RPMI) 1640 medium (Gibco BRL, Carlsbad, CA) supplemented with 10% heat-inactivated fetal bovine serum (FBS). Jurkat-tat cells were also supplemented with geneticin and hygromycin B, each at 0.5 mg per mL (Thermo Fisher Scientific, Walkersville, MD). TZM-bl cell line (obtained through the NIH AIDS Reagent Program, Germatown, MD, catalog number 8129) were cultured in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10% FBS.
Human tissues were obtained from routine surgery (unrelated to the current study) and according to all relevant ethical regulations for work with human participants including the patient’s informed consent. Tonsillectomies were performed in the Children’s Hospital (Washington, DC). Tissues were received from the Pathology Department and were considered as “pathological waste”. Tissue samples were anonymized and the protocol was approved by the Children’s Hospital IRB and by the NIH Office of Human Subject Research. Cervico-vaginal tissues were received as anonymized samples from the National Disease Research Interchange (NDRI). NDRI maintains a Federal Wide Assurance (FWA00006180) agreement with the DHHS, Office for Human Research Protections to comply with federal regulations concerning research involving human subjects. NDRI’s human tissue procurement programs and informed consent/authorization documents were approved by the IRB#5 of the University of Pennsylvania.
Tissues were dissected into 2-mm3 blocks, placed onto collagen sponge gel (Gelfoam, Pfizer, New York, NY) at the air–liquid interface, and cultured in RPMI 1640 medium supplemented with FBS at 15%, 1 mM non-essential amino acids, 1 mM sodium pyruvate, amphotericin B at 2.5-μg per mL, and gentamycin sulfate at 50-μg per mL25.
Antiviral activities of Lactobacillus-derived EVs were investigated in human cell lines and in human tissues ex vivo. A prototypic X4 HIV-1 isolate, LAI.04 (HIV-1LAI.04; Rush University Virology Quality Assurance Laboratory, Chicago, IL), and a prototypic R5 HIV-1 isolate, BaL (HIV-1BaL; Rush University Virology Quality Assurance Laboratory), were used.
To test the anti-HIV-1 effect in human cell lines, 50 μL of HIV-1LAI.04 (stock 350-ng p24gag per mL) or HIV-1BaL (stock 120-ng p24gag per mL) were preincubated with 50 μL of bacterial EVs derived from L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, or L. gasseri BC13 (stocks concentrated at 1 × 1010 EV per mL), with particles isolated from MRS medium, or with PBS (control), for 1 h, at 37 °C. We then infected 5 × 105 MT-4 (CXCR4+) or Jurkat-tat (CCR5+) cells with the EV/HIV-1LAI.04 or EV/HIV-1BaL mixture, respectively, for 1 h at 37 °C under agitation (400 rpm). After infection, cells were washed with 10 mL of PBS and centrifuged for 5 min at 400 × g to wash off all free virions. The pellet of infected cells was resuspended in 5 mL of RPMI 1640 medium either containing or not containing bacterial EVs (5 × 108 particles per mL, corresponding to ~1000 EVs per cell) and transferred to a 24-well plate (1 mL per well; Sigma-Aldrich, St. Louis, MO). MT-4 and Jurkat-tat cells were, respectively, cultured for 3 or 5 days, at 37 °C.
A similar type of experiments as above were conducted to address the concentration-dependent antiviral activity of EVs, choosing EVs released from L. gasseri BC12 as a model condition. Cells infected with EV/HIV-1LAI.04 or EV/HIV-1BaL were cultured in medium containing or not containing 5 × 104, 5 × 105, 5 × 106, 5 × 107, or 5 × 108 bacterial EVs per mL.
For human ex vivo tissues, either HIV-1LAI.04 or HIV-1BaL viral stocks were pretreated with Lactobacillus-derived EVs, MRS-derived particles, or PBS as mentioned above for 1 h at 37 °C. For HIV-1 infection in human tonsillar tissues ex vivo, nine blocks per well were placed on collagen sponge gel and infected with 15 μL of EV/ HIV-1 or EV-free/HIV-1 mixture on the top of each block. HIV-1BaL-infected tonsillar tissues were cultured in tissue culture medium containing or not containing 5 × 108 EVs per mL derived from L. crispatus (BC3 or BC5) and L. gasseri (BC12 or BC13). In contrast, cervico-vaginal ex vivo tissues were infected with 500 μL of EV/HIV-1BaL or EV-free/HIV-1 mixture for 2.5 h at 37 °C in agitation. Afterward, the infected cervico-vaginal tissue blocks were washed three times with PBS and transferred at the liquid–air interface onto Gelfoam (nine blocks per well). All tissue cultures ex vivo were kept for 12 days at 37 °C, replacing with the medium containing or not containing bacterial EVs (5 × 108 particles per mL) every 3 days.
The concentration-dependent antiviral activity of EVs derived from L. gasseri BC12 was tested in tonsillar and cervico-vaginal ex vivo tissues. Tissues infected with HIV-1LAI.04 or HIV-1BaL were cultured in tissue culture medium containing tenfold serial dilutions of bacterial EVs (5 × 108, 5 × 107, 5 × 106, and 5 × 105 particles per mL). We used eighteen tissue blocks per each condition (nine tissue blocks per well).
In all the experiments, we evaluated HIV-1 replication by measuring the p24gag antigen released in tissue culture medium, using an immunofluorescent cytometric bead-based assay by Luminex47.
Viral entry/cell attachment assays
HIV-1 viral entry was evaluated in TZM-bl cells (obtained through the NIH AIDS Reagent Program, MD). We cultured 2 × 104 TZM-bl cells per well in 100 μL of complete DMEM medium in a 96-well black plate (Sigma-Aldrich, St. Louis, MO) for 6 h to ensure complete cell adhesion. Afterward, the medium was replaced with 90 μL of fresh medium containing diverse concentrations of EVs (5 × 105, 5 × 106, 5 × 107, or 5 × 108 particles per mL) derived from L. gasseri BC12, or 5 × 108 particles per mL of particles derived from MRS medium, and the cells were infected with 10 μL of HIV-1LAI.04 stock, overnight. After infection, the medium was replaced with medium containing different amounts of bacterial EVs and cultured at 37 °C for 3 days. To measure HIV-1LAI.04 entry/integration into the cell, we removed the cell culture medium and lysed the cells with 100 μL of 1X of Glo lysis buffer (Promega, Madison, WI). We added 100 μL of 2X substrate Bright Glo luciferase buffer (Promega, Madison, WI). After a 3-min incubation, we measured the luminescence with a Saphire 2 luminometer (Tecan, Switzerland).
To study viral attachment/entry to cells, we incubated 150 μL of MT-4 cell suspension (5 × 106 cells) with 150 μL of HIV-1LAI.04 in medium containing or not containing 5 × 108 EVs released by L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, L. gasseri BC13, or particles derived from MRS medium for 2 h at 4 °C. Then, the infected cells were washed extensively five times with 1 mL of RPMI medium to eliminate all free viral particles by centrifugation at 400 × g for 5 min. Afterward, cells were lysed with lysis buffer (PBS containing 1% Triton X-100, 20 mM tris HCl, 0.05% tween-20, and 30% bovine serium albumin), and viral attachment/entry into the cell was evaluated in the cell lysates from measurements of the viral p24gag protein with Luminex.
To study whether bacterial EVs enter into the host cells and alter host cell function to induce protection against HIV-1, either TZM-bl or MT-4 cells were treated with bacterial EVs derived from L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, L. gasseri BC13, and MRS-derived particles for 24 h, prior to HIV-1 infection, and then HIV-1 infectivity was evaluated. For TZM-bl cells, 2 × 104 cells per well were cultured in 100 μL of complete DMEM medium in a 96-well black plate (Sigma-Aldrich, St. Louis, MO) containing or not containing bacterial EVs at a concentration of 5 × 108 EV per mL, at 37 °C for 24 h. Afterward, the cells were infected with 10 μL of HIV-1LAI.04 stock and cultured at 37 °C for 3 days. To measure HIV-1LAI.04 replication, we removed the cell culture medium and lysed the cells with 100 μL of 1X of Glo lysis buffer (Promega, Madison, WI). We added 100 μL of 2X substrate Bright Glo luciferase buffer (Promega, Madison, WI). After a 3-min incubation, the luminescence was measured with a Saphire 2 luminometer (Tecan, Switzerland). For MT-4 cells, 1 × 105 per well were cultured in 1 mL of complete RPMI medium containing or not containing EVs in a 24-well plate (Sigma-Aldrich, St. Louis, MO), at 37 °C for 24 h. Then, MT-4 cells were infected with 10 μL of HIV-1LAI.04 stock and cultured at 37 °C for 3 days. We evaluated HIV-1LAI.04 replication by measuring the p24gag antigen released in the cell culture medium (Luminex).
HIV-1 capture using magnetic nanoparticles
Human monoclonal PG9 antibody (1 mg per mL; Polymun Scientific, Austria, AB015), which preferentially recognizes trimeric HIV-1 envelope protein (gp120), was coupled to 15-nm carboxyl-terminated magnetic iron oxide nanoparticles (MNPs) according to the manufacturer’s protocol (Ocean NanoTech, San Diego, CA).
To study the effect of Lactobacillus-derived EVs on HIV-1 itself, we pretreated 50 µL of HIV-1LAI.04 viral particles (stock 350-ng per mL p24gag) with 50 µL of bacterial EVs derived from L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, and L. gasseri BC13 (stocks concentrated at 1 × 1010 EV per mL), with particles isolated from MRS medium or with PBS (control), for 1 h at 37 °C.
Afterwards, HIV-1 viral particles were captured with 50 µL of PG9-MNP-anti-gp120 antibody (stock 1 mg per mL) for 1 h, at 37 °C. We then separated HIV-1 virions captured by MNPs from the non-captured ones using magnetic columns attached to a high field MACS magnet (Miltenyi Biotech, Auburn, CA). After washing columns three times with 600 µL of washing buffer (0.5% bovine serum albumin, 1 mM ethylenediaminetetraacetic acid), we removed the MNP–HIV-1 complexes from the magnet, demagnetized them for 5 min, and eluted them with 600 µL of lysis buffer (PBS containing 1% Triton X-100), and measured the concentrations of HIV-1 p24gag antigen using an immunofluorescent cytometric bead-based assay by Luminex.
Cell viability and cell depletion assays
We performed cell viability assays in MT-4 and Jurkat-tat cells using the NucleoCounter® NC-100™ automated cell counting system (ChemoMetec, Denmark). We determined the numbers of total and dead cells in control cultures and in each Lactobacillus-derived EV-treated cultures (L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, L. gasseri BC13, 5 × 108 particles per mL) after 3 days of culture, using a propidium-iodide-based assay according to the manufacturer’s protocol (ChemoMetec, Denmark). We also tested the effect of particles derived from MRS bacterial medium (5 × 108 particles per mL) as described above. Triton X-100 at 0.2% was used in our study as a potent cytotoxic agent.
We also measured cell viability using the MTT (3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide) tetrazolium reduction kit according to the manufacture’s protocol (Sigma-Aldrich, St. Louis, MO). The MTT assay measures the mitochondrial dehydrogenase activity of living cells. Briefly, after day 3 of cell cultures (treated or not treated with EVs), 10 μL of MTT solution was added to each well (10% of culture volume) and plates were incubated for 4 h at 37 °C. After the incubation period, to dissolve the formazan crystals we added MTT solvent at 100 μL per well and incubated the plates for 1 h. After ensuring that the formazan crystals were dissolved, we measured the absorbance at 570 nm on Tecan Sapphire 2 using Magellan 5.0 software (Tecan Group Ltd., Switzerland).
We evaluated cell depletion on MT-4 cells treated or not treated with bacterial EVs (derived from L. gasseri BC12, 5 × 108 particles per mL) using flow cytometry. After 3 days of culture, the cells were centrifuged at 400 × g, resuspended in 1 mL of staining buffer (PBS containing 2% mouse serum, 2% goat serum, and 2% FBS), and stained with 1 μL of live/dead Fixable Viability Dye eFluor 450 (ef 450, Invitrogen, Carlsbad, CA) for 20 min. After incubation, cells were washed and further diluted with staining buffer and stained with anti-CD3-AF488 (Thermo Fisher Scientific, Waltham, MA, MHCD0320) and anti-CD4-BV605 (BD Bioscences, San Jose, CA, 562658) fluorescence-labeled monoclonal antibodies for 20 min. Data were acquired with a Novocyte flow cytometer (ACEA Biosciences, CA) equipped with 405, 488, and 650 nm laser lines. We analyzed the data using NovoExpress version 1.2.4 software (ACEA Biosciences, CA).
Protein extraction, SDS-PAGE, and western blotting
Total proteins were extracted either from bacterial EVs or from HIV-1-infected/non infected MT-4 cells treated or not treated with bacterial EVs, using RIPA Lysis and Extraction Buffer (Thermo Fisher Scientific, Waltham, MA). We loaded 10 μg of proteins on a 4–20% precast polyacrylamide gel (Bio-Rad Laboratories, Hercules, CA), separated them using SDS-PAGE, and then transferred them to low-fluorescence PVDF membranes and probed them with anti-HIV-1 p24 (0.5 μg per mL; Abcam, Cambridge, MA, ab9071), anti-p53 (1 μg per mL; Thermo Fisher Scientific, Waltham, MA, MA5-12557), anti-CD63 (1 μg per mL; Thermo Fisher Scientific, Waltham, MA, 10628D), anti-TSG101 (1 μg per mL; Thermo Fisher Scientific, Waltham, MA, MA1-23296), primary anti-mouse monoclonal antibodies, and then goat peroxidase-conjugated anti-mouse IgG secondary antibody (Bio-Rad Laboratories, Hercules, CA). We detected peroxidase activity and digital images using the ChemiDoc™ MP Imaging System (Bio-Rad Laboratories, Hercules, CA).
We subjected 500 μL of EVs (stocks concentrated at 5 × 1010 particles per mL) released by L. crispatus BC3, L. crispatus BC5, L. gasseri BC12, or L. gasseri BC13, or particles isolated from MRS medium, to a water bath sonication for 15 min to ensure complete EV lysis preceding 1H-NMR spectroscopy analysis. 1H-NMR spectra were recorded at 298 K with an AVANCE spectrometer (Bruker, Milan, Italy) operating at a frequency of 600.13 MHz, equipped with an autosampler with 60 holders48. Each spectrum was acquired using 32 K data points over a 7211.54-Hz spectral width and adding 256 transients A recycle delay of 5 s and a 90° pulse of 11.4 s were set up. The signals originating from large molecules were suppressed by a CPMG filter of 400 echoes, generated by 180° pulses of 24 μs separated by 400 μs. The signals were assigned by comparing their multiplicity and chemical shift with Chenomx software data bank (ver 8.1 Chenomx, Inc., Edmonton, Canada). We looked for features of the metabolome related to antiviral activity by evaluating the Pearson correlation between such activity and the concentration of each molecule identified. For this purpose, the function corr.test from the R (www.r-project.org) was employed. To highlight any overall trend characterizing the samples, we used the molecules whose concentration was significantly correlated to antiviral activity (p < 0.05) as a basis for a robust principal component analysis (rPCA) model49. For each model, we calculated the scoreplot, i.e., the projection of the samples in the principal components (PC) space, tailored to highlight the underlying structure of the data. Besides, we ranked the importance of each molecule in determining each PC. We did this by calculating how the coefficients attributed to each of them to determine each PC correlated, according to Pearson, with its concentrations.
Mass spectrometry of bacterial EVs
EVs (50 μL, from stocks at 5 × 1010 particles per mL) isolated either from L. gasseri BC12 or L. crispatus BC5 were analyzed for proteomics with mass spectroscopy (NICHD Biomedical Mass Spectrometry Facility, Bethesda, MD). Frozen EV samples were suspended in 0.1 M ammonium bicarbonate and solubilized with 0.2% ProteaseMAX (Promega Corp, Madison, WI) surfactant. Proteins were reduced with dithiothreitol and alkylated with iodoacetamide, before digestion overnight with sequencing grade trypsin (Promega Corp., Madison, WI). The digestion was quenched with 1 volume of 5% formic acid:acetonitrile (1:1), dried under vacuum, and reconstituted in 0.1% formic acid:acetonitrile (1:1). We analyzed the resulting peptides with LC-ESI-MS/MS using a 6560 IM Q-TOF mass spectrometer (Agilent Technologies, Santa Clara, CA) equipped with a Jet Stream Electrospray ionization source. We injected and separated aliquots of digested samples using reversed phase C18 gradient chromatography and collected MS/MS fragment spectra in a data dependent mode. We extracted tandem mass spectra from each run in Mascot Generic Format (MGF) and analyzed them using Mascot (Matrix Science, London, UK; version 2.6.2) searching the Eubacteria subset of the Sprot 2018_11 protein database (333,732 sequences) and a reverse sequence decoy database to determine the false discovery rate (FDR). Digestion enzyme specificity was set for trypsin with a maximum of 2 missed cleavages. The parent and fragment mass tolerances were set at 5 ppm and 0.05 Da respectively; carbamidomethyl (C) was set as a fixed and oxidation (M) as a variable modification. Scaffold (ver 4.8.7; Proteome Software Inc., Portland, OR) was used to validate MS/MS based peptide and protein identifications50. Peptide identifications were accepted if they could be established at >95.0% probability as specified by Peptide Prophet51. We assigned protein probabilities using the Protein Prophet algorithm (Nezvizhskii, 2003) and accepted protein identifications if they could be established at a 5% FDR and inclusive of at least two identified peptides. We obtained GO annotations for identified proteins using Scaffold with data imported from the NCBI website.
We performed all statistical analyses, unless otherwise specified, using the ordinary one-way ANOVA test (multiple comparison with Dunnett’s correction; GraphPad Prism version7; GraphPad Prism Software Inc., San Diego, CA). Results were expressed as means ± standard error of mean, and differences were deemed significant for p-values < 0.05.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
The data that support the findings of this study are available from the corresponding author L.M. upon reasonable request. The source data underlying Figs. 1b–d, 2a–c, 3a–b, 4a–c, 5a–b, 6, 7a–b, 9a–b, and Supplementary Fig. 1, are provided as a Source Data file. The mass spectrometry data have been deposited to the Mass spectrometry Interactive Virtual Environment (MassIVE) database (dataset identifier MSV000084514).
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This work was supported by the Intramural Research Program of the Eunice Kennedy Shriver National Institute of Child Health and Human Development, National Institutes of Health. We thank the Department of Pathology of Children’s National Medical Center for providing us with human tonsillar tissues.
The authors declare no competing interests.
Peer review information Nature Communications thanks Adam Burgener, Richard Ferrero and Fatah Kashanchi for their contribution to the peer review of this work. Peer reviewer reports are available.
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Ñahui Palomino, R.A., Vanpouille, C., Laghi, L. et al. Extracellular vesicles from symbiotic vaginal lactobacilli inhibit HIV-1 infection of human tissues. Nat Commun 10, 5656 (2019). https://doi.org/10.1038/s41467-019-13468-9
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