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Increased genital mucosal cytokines in Canadian women associate with higher antigen-presenting cells, inflammatory metabolites, epithelial barrier disruption, and the depletion of L. crispatus



Cervicovaginal inflammation has been linked to negative reproductive health outcomes including the acquisition of HIV, other sexually transmitted infections, and cervical carcinogenesis. While changes to the vaginal microbiome have been linked to genital inflammation, the molecular relationships between the functional components of the microbiome with cervical immunology in the reproductive tract are understudied, limiting our understanding of mucosal biology that may be important for reproductive health.


In this study, we used a multi’-omics approach to profile cervicovaginal samples collected from 43 Canadian women to characterize host, immune, functional microbiome, and metabolome features of cervicovaginal inflammation. We demonstrate that inflammation is associated with lower amounts of L. crispatus and higher levels of cervical antigen-presenting cells (APCs). Proteomic analysis showed an upregulation of pathways related to neutrophil degranulation, complement, and leukocyte migration, with lower levels of cornified envelope and cell-cell adherens junctions. Functional microbiome analysis showed reductions in carbohydrate metabolism and lactic acid, with increases in xanthine and other metabolites. Bayesian network analysis linked L. crispatus with glycolytic and nucleotide metabolism, succinate and xanthine, and epithelial proteins SCEL and IVL as major molecular features associated with pro-inflammatory cytokines and increased APCs.


This study identified key molecular and immunological relationships with cervicovaginal inflammation, including higher APCs, bacterial metabolism, and proteome alterations that underlie inflammation. As APCs are involved in HIV transmission, parturition, and cervical cancer progression, further studies are needed to explore the interactions between these cells, bacterial metabolism, mucosal immunity, and their relationship to reproductive health.

Video Abstract


Cervicovaginal inflammation, typically defined as elevated levels of pro-inflammatory cytokines, has been linked to increased rates of acquisition for sexually transmitted infections (STIs) including human immunodeficiency virus (HIV), diminished efficacy of topical pre-exposure prophylaxis (PrEP) for HIV prevention, cervical carcinogenesis, preterm birth, and long-term reproductive health complications such as pelvic inflammatory disease and tubal infertility [1,2,3,4,5,6,7,8,9,10,11,12,13,14,15]. Sustained inflammation can lead to increases in proteolytic enzymes, cause damage to the cervicovaginal epithelial barrier, and lead to increased immune cell infiltration or activation, which are thought to be potential mechanisms that increase the risk of HIV acquisition and lead to poor prognosis in cervical cancer [4, 16,17,18,19,20]. While many factors can modulate cervicovaginal inflammation including STIs and hormonal birth control, the vaginal microbiome is a major contributor [1, 21,22,23]. However, the relationships between the microbiome, mucosal immunity, and cervicovaginal inflammation are not well understood.

Epithelial and immune cells present in the cervicovaginal mucosa monitor the local microenvironment and initiate the production of cytokines and chemokines such as interleukin (IL)-1β, IL-6, and IL-8, and the recruitment or activation of leukocytes [24, 25]. The cervicovaginal mucosa is populated with a dynamic population of innate and adaptive immune cells including neutrophils, macrophages and monocytes, natural killer (NK) cells, T cells, and B cells [24,25,26]. The cervicovaginal immune system typically exists in homeostasis with the local microbiota [6, 27]. Typically the optimal vaginal microbiome is dominated by species of Lactobacillus, which are associated with low levels of inflammation, including low levels of pro-inflammatory cytokines such as IL-1, IL-8, tumor necrosis factor alpha (TNFα), and interferon gamma (IFNγ) [1, 23, 27,28,29]. Vaginal microbial dysbiosis, defined by a loss of Lactobacillus and an overgrowth of obligate and facultative anaerobes such as Gardnerella, Atopobium, or Mobiluncus [30,31,32,33,34], can also affect the mucosal microenvironment and have been associated with increases in pro-inflammatory cytokines, including IL-1β, IL-6, IL-8, and TNFα, resulting in recruitment, maturation, and activation of antigen-presenting cells (APCs), neutrophils, and CD4+ T cells [3, 4, 27,28,29, 35,36,37,38,39,40,41,42,43,44,45,46,47,48,49]. Indeed, the composition of the microbiome has been shown to be strongly associated with genital inflammation [3]. The modulation of inflammation is thought to be, in part, driven by metabolites derived from dysbiotic bacterial communities, such as short-chain fatty acids, amino acids, lipids, carbohydrates, and xenobiotics [6, 8, 50,51,52,53,54]. Conversely, lactate, produced by vaginal Lactobacillus, elicits anti-inflammatory effects from cervicovaginal epithelial cells, including suppression of IL-6, IL-8, and TNFα production [55, 56]. While these studies have provided insight into how the vaginal microbiome may modulate specific aspects of inflammation, the relationships between pro-inflammatory cytokines, resident immune cells, metabolites, and epithelial barrier function have been understudied limiting our understanding of potential mechanisms contributing to infectious disease susceptibility and other negative reproductive health outcomes.

In this study, we used a multi’-omics approach to profile cervicovaginal samples collected from Canadian women to characterize host, microbiome, and metabolome features of cervicovaginal inflammation. Using an integrated Bayesian network approach, we identify novel interactions linking vaginal mucosal inflammation with differences in the metabolome, microbiome, and APCs which may be important for mucosal health in the female genital tract.

Materials and methods

Study population

Forty-three women were recruited from gynecology clinics in Winnipeg, Canada, as part of the Vaginal Mucosal Systems (VMS) study. Enrollment criteria included age over 18 years, HIV negative, and no current or suspected pregnancy. All women provided written informed consent and the study was approved by the Institutional Review Board at the University of Manitoba.

Data and sample collection

Socio-demographic, obstetric, and gynecological data was collected by structured questionnaire. Physicians performed pelvic examinations and collected an APTIMA multi-test swab, 2 mid-vaginal swabs (Starplex Scientific Inc., Etobicoke, ON, rayon swabs, stored dry until processing), cervicovaginal lavage (CVL), 2 endocervical cytobrush samples, and touched a pH strip to vaginal wall. The APTIMA swab was sent to CADHAM provincial laboratory in Winnipeg, Canada, for chlamydia and gonorrhea testing. All other samples were immediately stored on ice and transported to the lab within 3 h of collection.

Cervicovaginal lavage

CVL was collected by bathing the cervical os with 10mL of sterile phosphate-buffered saline (PBS). CVL was aliquoted and stored at −80°C until use.

Cytokine array

25μL CVL was analyzed using EMD Millipore’s MILLIPLEX MAP 30-plex Human Cytokine/Chemokine Magnetic Bead Panel following the manufacturer’s procedures. Samples were randomized across the assay plate, and 25 samples were randomly selected to be analyzed in duplicate. Cytokines and chemokines that were below the limit of detection in ≥40% of samples were removed from analysis. Cytokines below the limit of detection were imputed using half of the minimum detectable concentrations. A curated list of 10 inflammatory cytokines (interferon α2 (IFN-α2), interleukin (IL)-1α, IL-1β, IL-6, IL-8, IFN-γ inducible protein 10 (IP-10), monocyte chemoattractant protein 1 (MCP-1), macrophage inflammatory protein (MIP)-1α, MIP-1β, and Regulated upon Activation, Normally T cell Expressed and Secreted (RANTES)) [2, 4, 5] were used to define inflammation within this study.

Endocervical cytobrush

Cytobrushes were vortexed for 45 s in PBS to dislodge cells, washed twice in fresh PBS, and filtered twice prior to staining with an optimized antibody cocktail: CD19-APC (clone HIB19), CD56-PE-Cy7 (clone B159), CD4-APC-H7 (clone RPA-T4), CD3-v500 (clone UCHT1), CD8-BV605 (clone SK1), CD49d-PE-Cy5 (clone 9F10), CD14-PerCP-Cy5.5 (clone MφP9), CD16-Alexa700 (clone 3G8), CD15-BUV395 (clone HI98), Fixable viability stain 570 (all antibodies obtained from BD Biosciences). Samples were fixed in 1% paraformaldehyde prior to acquisition on an LSR II (BD Biosciences). Human peripheral blood mononuclear cells were used for staining controls and fluorescence minus one (FMO) controls. Data was analyzed using FlowJo v10 (Treestar).

Diagnosis of bacterial vaginosis

A wet mount microscopy slide was created using 30μL vaginal swab eluate and observed at 400× magnification for the presence of Clue cells [57]. A Whiff test was performed by mixing 30μL eluate with 30μL of 10% KOH, with detection of a strong amine odor indicating a positive result [57]. A pH strip that had been touched to the vaginal wall was used to measure vaginal pH. Discharge color and consistency were assessed by the study physician during pelvic exam. A participant was diagnosed with bacterial vaginosis (BV) if they had 3 out of 4 Amsel criteria present.

Sample preparation for proteomics analysis

CVL supernatants were prepared for mass spectrometry as previously described [58]. Briefly, BCA assay (Novagen) was used to quantify protein and then equal volumes were used. Samples were denatured with 8M urea, reduced using diothiothreitol, alkylated using iodoacetamide, and digested into peptides using trypsin. CVL pellets were collected by centrifuging 2mL CVL at 21,000×g for 5 min at 4°C. Pellets were resuspended in 350μL lysis buffer (2% SDS, 0.1 M dithiothreitol, 0.5 M HEPES), then 50μL 0.1 mm glass beads were added. Samples were vortexed, heated at 95°C for 5 min, then vortexed for 3 min. Samples were centrifuged at 3000 rpm for 3 min to pellet beads and cells, and the supernatant was transferred to a fresh tube on ice. This was repeated 3 times. Protein quantification was determined using 2-D Quant assay (GE Healthcare, NJ, USA), and protein was denatured using 8M urea, alkylated using iodoacetamide, then treated with benzonase solution (250 U/μL benzonase, 50 mM MgCl2, 50 mM HEPES), before being digested by trypsin. Peptides were cleaned of salts and detergents by reverse-phase liquid chromatography (LC) using the step-function gradient. Peptides were then quantified using a LavaPep Fluorescent Peptide and Protein Quantification Kit (Gel Company, CA, USA) following the manufacturer’s protocol. One microgram of peptide per sample was re-suspended in 2% acetonitrile with 0.1% formic acid submitted for nanoflow-liquid chromatography-tandem mass spectrometry (LC-MS/MS) analysis.

LC-MS/MS setup for proteomics analysis

Each sample was separately analyzed using a nano-flow Easy nLC 1000 connected in-line to a Q-Exactive Plus mass spectrometer with a nanoelectrospray ion source at 2 kV (Thermo Fisher Scientific, San Jose, CA, USA). The peptide samples were loaded (1 μg) onto a C18-reversed phase Easy Spray column (50 cm long, 75-μm inner diameter, 2-μm particles (Thermo Fisher Scientific, San Jose, CA, USA)) with 100% buffer A (2% acetonitrile, 0.1% formic acid) for a total volume of 10 μl, and then separated on the same column. Peptides were eluted using a linear gradient of 5–22% buffer B (98% acetonitrile, 0.1% formic acid) over 100 min, 22–32% buffer B for 15 min, 32–90% buffer B for 5 min, and a wash at 90% B for 10 min at a constant flow rate of 200 nl/min. Total LC/MS/MS run-time was about 180 min, including the loading, linear gradient, column wash, and the equilibration.

MS data acquisition

Dynamically choosing the top 15 abundant precursor ions from each survey scan for isolation in the quadrupole (1.4 m/z isolation width) and fragmentation by HCD (28% normalized collision energy). The survey scans were acquired in the orbitrap over m/z 375–1500 with a target resolution of 70,000 at m/z 200, and the subsequent fragment ion scans were also acquired in the orbitrap with a resolution of 17,500 at m/z 200. The lower threshold for selecting a precursor ion for fragmentation was 1.9e4. Dynamic exclusion was enabled using a list size of 500 features, a m/z tolerance of 15 ppm, a repeat count of 1, and an exclusion duration of 20 s.

Human proteome data analysis

Raw MS spectra were imported into Progenesis QI software (v2.0, Nonlinear Dynamics), aligned, and filtered as described previously [21, 59]. Filtered peptides were annotated using Mascot Daemon (v.2.4.0, Matrix Science) and searched against the SwissProt/UniProtKB (2015) human database, with a decoy database included to determine the rate of false discovery. Protein identifications were confirmed using Scaffold software (v4.8.3, Proteome Software) with confidence thresholds set at ≤1% FDR protein at the protein level, ≤0.1% FDR at the peptide level, and had ≥2 unique peptides identified per protein. Normalized relative abundances of each protein within each sample were obtained from Progenesis QI. Only proteins that had an average covariance of <25% (925 proteins) as determined through measurements of a standard reference sample run at 10 sample intervals (n=7) were used in downstream analysis to exclude proteins with higher technical measurement variability. Pathway analysis of host proteins was performed using ConsensusPathDB-human [60,61,62,63].

Microbial proteome data analysis

Protein database searches were conducted against an in-house vaginal metaproteome (VMP) database [64] using Mascot (v.2.4.0, Matrix Science) and included human proteins from the SwissProt/UniprotKB database to limit potential homologous identifications. Search results were then imported into Scaffold software to validate these protein identifications, filtered using the following criteria: <0.1%FDR for peptide identification, \(\le\) 1% FDR for protein identification, and at least two unique peptides identified per protein, and protein spectral counts were normalized to total protein detected. Microbial taxa abundance was estimated by taking the sum of normalized total spectral counts from Scaffold for all proteins associated with each genus. Scaffold accession reports containing homologous protein information were used to identify proteins that matched to more than one genus, which were binned into an “undistinguishable” category.

Functional microbiome analysis

Non-homologous bacterial proteins identified in each participant were annotated for known biological functions using the KEGG ontology database with GhostKOALA (v2.2, Kyoto University Bioinformatics Center) [65]. Proteins were binned to the pathway level; a total of 33 pathways were analyzed for interactions with inflammation to preserve experimental power.

Sample preparation for metabolomics analysis

Metabolomics procedures were adapted from Srinivasan et al. [52]. Metabolites were extracted from CVL using a 1:4 ratio of CVL to methanol, followed by vortexing and centrifugation at 16,000×g for 30 min at 4°C. The supernatants were transferred to new tubes and dried using vacuum centrifugation. Metabolite samples were resuspended in 200μL of sample buffer (30% Buffer A: 70% Buffer B containing 53.1 μM 13C5-15N1-glutamic acid and 58.2 μM 13C2-succinic acid. Buffer A = 5 mM ammonium acetate in 0.1% acetic acid, Buffer B = 0.1% acetic acid in acetonitrile), then vortexed for 15 min and centrifuged at 16,000×g for 30 min to remove particulate matter. A standard sample containing a mixture of 10 known metabolites, along with a mix sample consisting of extracted metabolites from a mixture of all samples, was injected periodically throughout each batch run for QC and monitoring LC-MS/MS conditions.

Targeted LC-MS/MS metabolomics analysis

Metabolites were separated using an Agilent 1200 binary pump HPLC system equipped with a ZIC-cHILIC column (150 × 2.1 mm, 3.0 μm particle size) (Millipore). The flow rate was set to 200 μL/min and the column temperature was kept at 4°C. The separation gradient was set as follows: 0–3 min: 70% B, 3–7.5 min: 70–30% B, 7.5–13.5 min: 30% B, 13.5–16.5 min: 30–70% B, 16.5–27 min: 70% B. Eight microliters of each sample was injected for simultaneous positive and negative mode analysis on a Fusion Lumos Tribrid mass spectrometer. Targeted quantification of metabolites was accomplished in parallel reaction monitoring (PRM) mode, targeting 121 different metabolites (66 in positive mode, 55 in negative mode). Source conditions for positive mode were set as follows: Spray Voltage: 3500 V, Sheath Gas: 3 (Arbitrary Units), Aux Gas: 1.2 (Arbitrary Units), Ion Transfer Tube Temp: 275°C. Source conditions for negative mode are the same as for positive except the Spray Voltage is set to 2100 V. Mass spectrometry data is acquired by alternating MS1 and MS2 scans in both positive and negative mode. MS1 scans are collected with the following parameters (the same for positive and negative unless listed otherwise): Scan range: 55–280 m/z (positive), 65–500 (negative), Orbitrap resolution: 30,000, RF Lens (%): 30, AGC Target: 4.0e5, Max Injection Time: 50 ms. MS2 scans are collected with the following parameters (the same for positive and negative mode unless listed otherwise): Isolation Window: 1.6 m/z, HCD Collision Energy: 30%, Stepped Collision Energy: +/− 10%, Orbitrap Resolution: 15,000, Maximum Injection Time 22 ms. For MS2 scans, the mass range was set from 50 m/z to the mass of the targeted metabolite + 10 m/z. Raw files obtained are subsequently uploaded into Skyline for metabolite peak integration and quantification using a custom method. A zero replacement strategy was used to impute values for metabolites below the limit of detection, and metabolites that were below the limit of detection in ≥40% of samples were removed from the analysis.

Statistical analysis

Statistical analysis and data visualization was performed with GraphPad Prism 8 (v.8.3.1 (332)) or R (version 4.1.3) with plugins “NMF” (version 0.24.0), “RColorBrewer” (version 1.1-2), “dendextend” (version 1.16.0), and “ggplot2” (version 3.3.5). Demographic and gynecological data was analyzed using chi-square or Kruskal-Wallis with Dunn’s multiple comparison test. Multi-‘omics data was analyzed using Kruskal-Wallis with Benjamini-Hochberg correction for multiple comparisons.

Bayesian Network analysis

Random forest models were created for each multi-‘omic dataset (vaginal metaproteome taxa, vaginal metaproteome functions, vaginal metaproteome proteins, metabolome, host proteome, cytokine, and flow cytometry) using the 3-level inflammation variable as the classifier. All continuous data was discretized using above/below median prior to network creation. Datasets were first screened using Random Forest models [66] in R (randomForest, version 4.7-1.1) to assess the top 5 most important variables based on Gini importance, which were selected as features for the network. The inflammation variable was also included in the network, resulting in 36 features chosen as nodes. Four participants were removed from this analysis as they did not have complete information across datasets. Discretized data from the 36 selected features across 39 participants were used as input for the Bayesian Network, which was constructed using the BNlearn package in R (version 4.8.1). To avoid getting stuck at a possible local maximum, 1000 networks were bootstrapped and averaged for 1000 random restarts, resulting in 1,000,000 total networks. The final consensus network was calculated using the function in BNlearn [67]. For each network created, the structure of the network was learned using the Hill-Climbing algorithm with the likelihood-equivalence Bayesian Dirichlet (BDe) scoring method. The optimal imagery sample size was calculated with the function. As the network is intended to be a hypothesis-generating tool, the presence of an edge describes a relationship between two nodes without directionality. The final graph was visualized in Gephi using the Fruchterman Reingold layout. The nodes are colored by data type and size indicates degree of the node.


Study participants

Forty-three women were recruited from gynecology clinics in Winnipeg, Canada, as part of the Vaginal Mucosal Systems (VMS) study. Most participants self-reported as Caucasian (37, 86%). Sixteen participants (37%) self-reported having at least 1 vaginal symptom in the past month, including discomfort, itchiness, discharge, or bleeding. Ten participants (23%) had cervical ectopy. Twenty-three (53%) reported intercourse in the past 30 days, with 2 (5%) reporting anal intercourse, and 9 (21%) reporting using condoms. Use of hormonal contraceptives was low, with 12 participants (30%) reporting use, primarily of intrauterine devices (IUDs). Twelve (28%) had a history of any sexually transmitted infection, with 1 participant testing positive for chlamydia at the study visit.

We classified participants into low, medium, or high genital inflammation groups (Table 1) based on the concentrations of 10 inflammatory cytokines in CVL that have been previously linked with increased acquisition of HIV (IFN-α2, IL-1α, IL-1β, IL-6, IL-8, IP-10, MCP-1, MIP-1α, MIP-1β, and RANTES) [2, 4, 5] using unsupervised hierarchical clustering (Fig. 1). Women in the low inflammation group (n=6) had a median of 0 (range 0–3) inflammatory cytokines in the upper quartile, while women in the medium inflammation group (n=25) had a median of 1 (range 0–3) inflammatory cytokines in the upper quartile, and women in the high inflammation group (n=12) had a median of 5 (range 2–10) inflammatory cytokines in the upper quartile. Vaginal pH was significantly lower (Kruskal-Wallis p=0.034, H statistic=6.75, Degrees of freedom=2) in the low inflammation group compared to the medium (p.adj=0.064) and high (p.adj=0.037) inflammation groups. There were no significant differences in age, Nugent score, bacterial vaginosis (BV) diagnosed using Amsel criteria, or Lactobacillus dominance of the microbiota (defined as >50% microbial proteins from Lactobacillus species) between groups (Table 1). IL-1β was the only cytokine that difference based on Lactobacillus dominance of the microbiome (p=0.021) and was increased in non-Lactobacillus dominant (nLD) participants.

Table 1 Overview of participant characteristics
Fig. 1
figure 1

Heatmap showing clustering of inflammation groups based on cytokine levels in cervicovaginal fluid of study participants. Inflammatory cytokines were quantified in CVL using Luminex technology. Unsupervised hierarchical clustering was used to group participants by low, medium, or high levels of inflammation. N=43

Antigen-presenting cells differ based on vaginal inflammation status

As vaginal inflammation has been associated with increased immune cell infiltration, we used multiparameter flow cytometry to phenotype endocervical immune cells collected from study participants to detect immune cell lineages (CD4+ T cells, CD8+ T cells, CD19+ B cells, CD56+ Natural Killer (NK) cells, CD14+ antigen-presenting cells (APCs), and CD15+CD16+CD49d- neutrophils) (Fig. 2A, Supplemental Figure 1). Neutrophils (mean 30.3% range 0.13–83.17%) were the most abundant immune cell present, followed by CD3+ T cells (mean 28% range 0.0–91.2%) and NK cells (mean 7.6% range 0.14–30.68%). When we examined immune cell differences based on inflammation status, APCs were the only cell type that differed by inflammation (Kruskal-Wallis p=0.025, H statistic=7.39, Degrees of freedom=2) (Fig. 2B), with significantly higher levels of APCs in participants in the medium compared to low inflammation groups (p.adj=0.03). No immune cell subsets differed by Lactobacillus dominance of the microbiome.

Fig. 2
figure 2

Flow cytometry analysis associates higher cervical antigen-presenting cells with increased genital inflammation. A Cervical leukocytes were immunophenotyped by flow cytometry to identify immune cell lineages. B APCs identified from cervical cytobrushes, stratified by inflammation level defined by the presence of inflammatory cytokines in CVL. Adjusted p values are reported and were calculated using the Kruskal-Wallis test with Dunn’s correction for multiple comparisons. Data is presented as a percentage of total live cells identified by flow cytometry with median identified. N=43

Vaginal inflammation is associated with proteome alterations related to increased innate immunity and decreased epithelial barrier integrity

Using mass spectrometry-based proteomics there were 925 human proteins identified within CVL. There were 275 (29.8%) proteins that were significantly different by inflammation group (p<0.05), with 81 (8.8%) passing correction for multiple comparisons (p.adj<0.05). These 81 proteins clustered by inflammation group using unsupervised hierarchical clustering (chi-square p<0.0001) into “high inflammation” and “medium/low inflammation” branches, and two main protein clusters were identified (Fig. 3). Cluster A contained 21 proteins, which are increased in all (11/11) participants with high inflammation and 36% (9/25) of the medium inflammation participants. Proteins in cluster A were associated with biological pathways related to innate immune system (p=2.26E−07), including neutrophil degranulation (p=1.75E−06), integrin signaling (p=5.83E−04), and leukocyte migration (p=1.37E−05), indicating there are higher proteome signals of inflammation in participants with higher levels of cytokine-defined inflammation. Cluster B contained 60 proteins, which tend to be lower in participants with high inflammation. Proteins within Cluster B are associated with tissue integrity pathways, including cell-cell adherens junction (p=1.94E−07), cornified envelope (p=4.52E−12), and keratinization (p=4.70E−05), indicating decreased epithelial barrier integrity or increased barrier disruption with high inflammation. The “high inflammation” branch, which had increases in proteome signatures related to innate immunity, contained participants that had significantly higher levels of neutrophils (p=0.0247), which supports the findings of the pathway analysis. While there were 134 host proteins that differed between Lactobacillus dominant (LD) and non-Lactobacillus dominant (nLD) groups, none passed correction for multiple comparisons.

Fig. 3
figure 3

Cervicovaginal inflammation associates with neutrophil and epithelial barrier proteome changes. Mass spectrometry analysis of cervicovaginal fluid identified alterations to the mucosal proteome with inflammation groups. Proteins that were differentially abundant (adj. p<0.05) underwent unsupervised hierarchical clustering, and inflammation status based on levels of inflammatory cytokines was overlaid. Two clusters of proteins were identified. Proteins from each cluster underwent pathway analysis using ConsensusPathDB-human and significant pathways are shown on the right. One participant (high inflammation group) did not have a sample available for mass spectrometry analysis. Differential protein expression analysis was performed using the Kruskal-Wallis test with Benjamini-Hochberg correction for multiple comparisons. N=42

L. crispatus is higher in participants with low genital inflammation

As it has been observed that the vaginal microbiome can have a significant impact on inflammation, we used mass spectrometry-based metaproteomics to detect bacterial proteins present in CVL. 1758 unique bacterial proteins from 19 genera were identified by mass spectrometry (Fig. 4). L. crispatus, L. iners, Gardnerella, and other Lactobacillus species were the most abundant bacteria detected. When participants were classified based on the abundance of Lactobacillus detected, with women having >50% of their bacterial proteins from Lactobacillus considered Lactobacillus dominant (LD), we found that all participants with low inflammation (6/6, 100%), 16 from the medium inflammation group (64%), and 7 from the high inflammation group (58%) were LD, although this was not statistically different (p=0.184). Relative abundance of L. crispatus was significantly different based on the inflammation group (Kruskal-Wallis p=0.004, H statistic=10.83, Degrees of freedom=2), and was higher in the low inflammation group compared to both the medium (p.adj=0.0064) and high (p.adj=0.0067) groups (Fig. 4C). Ruminococcus was also statistically different between inflammation groups (Kruskal-Wallis p=0.019 H statistic=7.93, Degrees of freedom=2), with a significant increase in medium compared to low inflammation (p.adj=0.020). However, this bacterium was in low abundance and the differences appeared to be driven by 3 participants that had higher levels of this bacteria. No other bacteria were significantly different between inflammation groups.

Fig. 4
figure 4

Cervicovaginal microbiome composition and functional differences between women with high and low genital inflammation. Proportion plots of A taxa and B ko-level bacterial functions identified in cervicovaginal lavage by mass spectrometry. Participants are grouped by inflammation status. Two participants in the medium inflammation group did not have bacterial functions mapped to the identified bacterial proteins. C Microbial proportion of L. crispatus grouped by inflammation status with median identified. D Proportion of ko-level bacterial functions by inflammation status. Pie charts show the distribution of bacterial taxa for each function. E Bacterial proteins that differed by inflammation status. Pie charts show the distribution of bacterial taxa for each protein. Adjusted p values are reported and were calculated using the Kruskal-Wallis test with Dunn’s correction for multiple comparisons. N=43

KEGG gene ontology was used to map the bacterial proteins to functional pathways, with 971 (55%) bacterial proteins mapped to 33 ko-level pathways. The most abundant functions were glycolysis/gluconeogenesis, carbon fixation, and RNA degradation. There were 5 ko-level pathways that were significantly different by inflammation group, inositol phosphate metabolism (p=0.002, p.adj=0.074), two-component system (p=0.007, p.adj=0.119), carbon fixation (p=0.014, p.adj=0.145), amino sugar and nucleotide sugar metabolism (p=0.018, p.adj=0.145), and fructose and mannose metabolism (p=0.041, p.adj=0.233), although none passed correction for multiple comparisons (Fig. 4D). There were 25 bacterial proteins identified that were significantly different by inflammation status, but none passed correction for multiple comparisons. Of these proteins, eight (glutamine synthetase, glyceraldehyde-3-phosphate dehydrogenase, glyceraldehyde-3-phosphate dehydrogenase type 1, phosphate binding protein, phosphoenolpyruvate carboxykinase (ATP), phosphoglucosamine mutase, triosephosphate isomerase, and uncharacterized protein) were present in the ko-level pathways that differed by inflammation group. Triosephosphate isomerase (p=0.0018), which was identified in the fructose and mannose metabolism, inositol phosphate metabolism, and carbon fixation pathways, was significantly lower in the high inflammation group compared to both the medium (p.adj=0.0336) and low (p.adj=0.0021) inflammation groups. Glyceraldehyde-3-phosphate dehydrogenase type 1 (p=0.0212), identified in the carbon fixation pathway, was the only protein that was higher in the high inflammation group compared to the low inflammation group (p.adj=0.0225) (Fig. 4E), suggesting a change in bacterial metabolism may be associated with increasing inflammation.

Vaginal xanthine is significantly higher in women with high levels of vaginal inflammation

To investigate potential communications between the host and the microbiome, we used targeted metabolomics to identify metabolites in CVL. A total of 82 metabolites were identified including amino acids, short chain fatty acids, organic acids, fatty acids, carbohydrates, nucleic acids, and amines. Eleven (13.4%) metabolites were significantly different based on the inflammation group (p<0.05, Kruskal-Wallis test; Fig. 5A), including fatty acids (4 metabolites), organic acids (2 metabolites), nucleic acids (2 metabolites), sugars (2 metabolites), and amino acids (1 metabolite). The purine nucleic acid xanthine was the top metabolite associated with inflammation (Kruskal-Wallis p=6.00E−4, BH p.adj=0.046, H statistic=14.99, Degrees of freedom=2), and is higher in both the medium (Dunn’s p.adj=0.033) and high (Dunn’s p.adj=0.0003) inflammation groups compared to women with low inflammation, and increased in the high group compared to the medium group (p.adj=0.076), although this did not pass statistical significance (Fig. 5B). Other metabolites increased in participants with high inflammation included hexose-phosphate (p=0.0115, p.adj=0.21), hexose (p=0.0274, p.adj=0.28), N-acetyl alanine (p=0.0471, p.adj=0.33), 12-hydroxyeicosatetraenoic acid (p=0.0125, padj=0.21), and 13-hydroxyoctadecadienoic acid (p=0.0331, p.adj=0.28), although none passed correction for multiple comparison. Metabolites that were higher in participants with low inflammation included homovanilate (p=0.0125, p.adj=0.21), lactate (p=0.034, p.adj=0.28), adenosine (p=0.0075, p.adj=0.21), and succinate (p=0.0207, p.adj=0.28), although none passed correction for multiple comparisons (Fig. 5C). Interestingly, phenyllactate (p=0.0233, p.adj=0.28) was lowest in the participants with medium inflammation. Unsupervised hierarchical clustering indicated these metabolites tended to cluster by inflammation group (chi-square p=0.101) and did not cluster by Lactobacillus dominance of the microbiome (Fisher’s exact p=0.469). There were 26 (31.7%) metabolites that differed based on microbiome status, with 14 (cytosine p.adj=0.033; inosine p.adj=0.033; glycine p.adj=0.033; lactate p.adj=0.033; methionine sulfoxide p.adj=0.033; tyrosine p=0.034; adenosine p.adj=0.034; serine p.adj=0.036; uridine p.adj=0.039; tryptophan p.adj=0.039; hexose p.adj=0.047; glutamate p.adj=0.047; leucine-isoleucine p.adj=0.047; xanthine p.adj=0.047) passing correction for multiple comparisons. Of these 14 metabolites, 3 overlapped with the inflammation metabolomic signature (xanthine, adenosine, and lactate) suggesting these metabolites may be important for microbiome-inflammation interactions (Supplemental Table 1).

Fig. 5
figure 5

Cervicovaginal metabolome differences between women with high and low inflammation. A Hierarchical clustering of differentially abundant (p<0.05) metabolites based on inflammation group. B Log2 normalized abundance of xanthine identified in CVL samples by inflammation group with median indicated. C Log2 normalized abundance of lactate identified in CVL samples by inflammation group with median indicated. Adjusted p values are reported and were calculated using the Kruskal-Wallis test with Dunn’s correction for multiple comparisons. Two participants from the high inflammation group did not have samples available for metabolomics analysis. N=41

Bayesian network analysis identifies molecular relationships with inflammation

To better understand the potential relationships between cervicovaginal inflammation and the microenvironment, we employed an integrated Bayesian network method. The cytokine, immune cell, proteome, metaproteome (species, functional pathway (b level), protein), and metabolome datasets were pre-filtered using random forest models, and the top 5 features were selected from each dataset, with the inflammation variable also included, leading to a total of 36 features. The final model identified 119 edges between 36 nodes (Fig. 6A). Inflammation, L. crispatus, and succinate were major nodes identified. Inflammation status was related to the neutrophil chemotactic factor IL-8, pro-inflammatory cytokine IL-1β, and to APCs. Primary interactions with inflammation status included links to epidermal integrity proteins (SCEL and IVL), as well as metabolites, including xanthine and carbohydrates hexose and hexose-phosphate. Primary microbiome interactions included anaerobic taxa Prevotella and Ruminococcus. A second major node identified was L. crispatus, which was linked to L. iners and Gardnerella. L. crispatus was also directly linked to the inflammatory cytokine MIP-1α, and the immune cells APCs, neutrophils, and CD4+ T cells. Succinate is a metabolite that has been associated with BV, and was linked to both L. crispatus and Gardnerella in this network. While succinate was not linked directly to inflammation, it was linked to MIP-1α and APCs. Succinate was also linked to bacterial carbohydrate metabolism, carbohydrate metabolites, and the human protein SCEL, which is part of the cornified envelope. When metabolites, microbiome features, and host proteins were classified as above or below median levels and underwent unsupervised hierarchical clustering, we found that samples cluster by inflammation (chi-square p=5.34 × 10−5) and level of APCs (FET p=0.031) (Fig. 6B), indicating a potential shift in metabolic pathways with increases in inflammation, which was also reflected in shifts in bacterial metabolism based on the bacterial proteome. Overall, this network highlights several novel interactions between APCs, metabolites, and bacterial functions that may be important for mediating cervicovaginal inflammation.

Fig. 6
figure 6

Bayesian network analysis of cervicovaginal inflammation. Major features are colored by dataset. Node size is representative of the number of edges per node, with larger nodes having more edges (A). Heatmap of the top five features selected by Random Forest based on Gini importance from host proteome, microbiome, bacterial protein, and metabolome datasets (B). Each feature was assigned to above or below median level and used for unsupervised hierarchical clustering. Inflammation status and levels of APCs are overlaid. Samples significantly cluster by inflammation status (chi-square p=5.34 × 10−5). Pie charts show the distribution of bacterial taxa for each protein included in the heatmap


Sustained cervicovaginal inflammation can have a detrimental impact on the cervicovaginal mucosa, leading to epithelial barrier damage and increased immune cell infiltration or activation, resulting in adverse health outcomes. In this study of women living in Canada, we show that APCs are significantly higher with vaginal inflammation and linked to the microbiome, the metabolite succinate, loss of functional bacterial pathways, epithelial barrier disruption, and neutrophil-related activation pathways. In addition, we identified the metabolite xanthine as another key feature of increased inflammation. Overall, this study shows a complex interplay between shifts in bacterial metabolism to increased pro-inflammatory cytokines and changes to innate immunity in the female genital tract.

APCs are important sensors of the local microenvironment, linking innate and adaptive immunity. Work by others has found that APC frequency is not significantly different based on microbiome group, but that there are pronounced transcriptional differences in cervical APCs from women with Lactobacillus compared to non-Lactobacillus microbiomes [27, 68]. APCs from women with non-Lactobacillus microbiomes exhibited upregulation of pro-inflammatory mediators including TNFα signaling pathways and increased expression of pro-inflammatory cytokine genes compared to Lactobacillus dominant women [27, 68]. These APCs were also more activated and mature, which could contribute to subsequent T cell priming and control of effector functions [27]. In this study, we did not observe any difference in APC levels based on Lactobacillus dominance but there was a relationship between APCs and lower L. crispatus. There were no significant correlations between non-Lactobacillus microbiota and APCs, which may be due to the lower levels of these bacteria in this cohort. APCs were also linked to the metabolite succinate, which was identified as a major molecular feature of inflammation. Succinate has previously been linked to BV [52] which agrees with our findings that succinate associates with L. crispatus, Gardnerella, and Ruminococcus. Succinate is a pro-inflammatory metabolite and can augment TLR-induced production of TNF and IL-1β and trigger chemotaxis and activation of APCs [69, 70]. In addition, succinic acid can significantly increase HIV expression in infected macrophages and increase IL-8 production by virus-infected cells [71]. Thus, succinate could be a metabolite linking the vaginal microbiome to APCs and subsequent inflammation in the cervicovaginal mucosa. As subsets of APCs can be infected by HIV and have been associated with both parturition [72,73,74,75,76] and progression of solid tumors, including cervical cancer [16, 77,78,79,80], this interaction between inflammation, the microbiome, and metabolites could be an important component of reproductive health.

Proteomics analysis confirmed the inflammation grouping of participants, with those having high inflammation having increases in pathways related to immune cell infiltration, phagocytosis, and neutrophil degranulation. Interestingly, APCs were the only immune cell increased in participants with high inflammation, suggesting that higher levels of inflammation may represent functional or phenotypic changes in immune cell subsets that may not be reflected by immune cell lineage analysis. Follow-up studies are further characterizing cervical immune cell populations to investigate functional differences that may exist. Participants with high levels of inflammation also had decreases in pathways related to epithelial barrier integrity, which supports a relationship between increased inflammatory cytokines and epithelial barrier damage. Indeed, we have previously shown that elevated levels of cytokines were associated with mucosal proteome signatures of decreased barrier proteins [4]. Inflammation was directly linked to the barrier proteins sciellin (SCEL), serpin B3 (SERPINB3), and involucrin (IVL). While there were no direct links identified between these proteins and the microbiome in our analysis, they did link to bacterial functions such as carbohydrate metabolism and signal transduction, and to metabolites including succinate, xanthine, and hexose-phosphate, suggesting an indirect link between barrier damage and the microbiome via bacterial metabolism.

The microbiome can be a major contributor to mucosal inflammation [6]. L. crispatus was significantly higher in participants with low inflammation compared to both the medium and high inflammation groups, which supports the findings of other studies [1, 10, 14,15,16]. Inflammation was directly linked to Prevotella and Ruminococcus. Prevotella has a recognized role in BV and is linked to inflammation and increased cytokine production [81] and has been linked to increased inflammation in other studies [1, 27, 28, 68]. In mouse models, vaginal introduction of Prevotella increased IL-6 and IL-8 production and recruited and activated CD4+ T cells in the genital mucosa compared to L. crispatus inoculation [21]. Prevotella was linked directly to neutrophils and IP-10, suggesting these are potential mediators of Prevotella-associated inflammation. Ruminococcus has been identified in the vaginal microbiota in other studies [64, 82], but its role in inflammation has not been studied. Ruminococcus was linked directly to IL-1β and CD8+ T cells, although directionality of this is not known, so it is difficult to determine the effect of Ruminococcus on inflammation. In addition, Ruminococcus was a low-abundance bacterial species identified, suggesting larger studies are needed to better understand its potential role in the cervicovaginal microenvironment.

The functional metaproteomic data indicated changes in bacterial metabolism associated with inflammation. Interestingly, lactate and bacterial enzymes such as lactate dehydrogenase, which are typically associated with low inflammation [28, 56, 83, 84], were not among the top features selected, whereas triosephosphate isomerase, detected primarily from L. crispatus, was selected. This suggests that enzymes involved upstream of homolactic fermentation may be better indicators or more important contributors to metabolic stability that are needed to maintain low levels of inflammation. This information may be helpful for the design of microbiome-based therapeutic interventions that are targeting the vaginal microbiome and selection parameters for L. crispatus strains for inclusion in these interventions. Inositol phosphate metabolism was also significantly decreased in participants with high inflammation. Microbiota-derived inositol phosphate has been found to regulate histone deacetylase (HDAC) activity in the gut, with commensal bacteria stimulating HDAC activity through inositol triphosphate production and promoting epithelial repair in a mouse model of colitis [85, 86]. In support of this, we found that high inflammation associated with decreased human pathways of epithelial barrier integrity, including significant decreases in the keratinocyte-associated proteins IVL and SCEL.

Xanthine was identified as a major metabolite underlying increased inflammation. Xanthine is a purine base that is found in most human tissues and fluids and its role in inflammation is not well studied, although it has been demonstrated to be increased in amniotic fluid following LPS exposure in mouse models and increased in women that had a spontaneous first-trimester miscarriage [87, 88]. Xanthine is a degradation product of inosine, which has been studied in the context of both the gut microbiome and immunity [89, 90]. Increases in microbiome-derived inosine can promote antitumor immunity, which is dependent on the activation of CD4+ Th1 cells [89]. While increased levels of xanthine were also observed in this study, mechanistic experiments were only performed with inosine [89]. In addition, effector CD8+ T cells can utilize inosine to support cell growth and function in the absence of glucose in vitro [90]. While inosine was detected by metabolomics in this study, it was not associated with inflammation status. Future studies should investigate the impact of both xanthine and inosine on cervicovaginal T cell function.

A major strength of this study is the in-depth multi-‘omics analysis that was performed, including cytokines, multiparameter flow cytometry, metaproteomics, and metabolomics on paired samples, allowing us to undertake more complex analysis such as Bayesian network to investigate potential interactions. While the Bayesian network analysis is descriptive and allows the identification of potential relationships for future mechanistic studies, several of the interactions identified support published data. In addition, this study investigated cervicovaginal inflammation in participants that would be considered healthy, illustrating potential factors that could contribute to an inflammatory microenvironment in the absence of disease. Limitations of this study include the small sample size and lack of microbiome diversity, with only 8 participants (19%) having a clinical diagnosis of BV, which is a major modulator of the cervicovaginal microenvironment. In addition, CD45, as a marker of hematopoietic-derived immune cells, was not included in the flow cytometry panel. While this precludes CD45 vs SSC gating, which could impact the identification of leukocyte subsets within samples, all immune cell subtypes were identified using lineage-specific markers. Finally, data on the menstrual phase and menopause was not collected. As there was no upper age limit for recruitment into this study, the average participant age was high, and it is likely that several participants had reached menopause. While it is important to study the impacts of age or menopause on the cervicovaginal microenvironment, the hormonal and microbiome changes that occur over the menstrual cycle and with menopause may confound the findings.

In conclusion, this study identifies interactions between microbial metabolism and the cervicovaginal microenvironment that could modulate inflammation and host immunity. These data may have implications for susceptibility to infections in the female genital tract and other reproductive health outcomes. Further studies are needed to explore the interactions between bacterial metabolism, mucosal immunity, APCs, and genital inflammation.

Availability of data and materials

Data sets including cytokine measurements, immune cell levels, metaproteome, and metabolome have been included as a supplemental file.


  1. Lennard K, et al. Microbial composition predicts genital tract inflammation and persistent bacterial vaginosis in South African adolescent females. Infect Immun. 2018;86:1–18.

  2. Masson L, et al. Genital inflammation and the risk of HIV acquisition in women. Clin Infect Dis. 2015;61:260–9.

    Article  PubMed  PubMed Central  Google Scholar 

  3. Gosmann C, et al. Lactobacillus-deficient cervicovaginal bacterial communities are associated with increased HIV acquisition in young South African women. Immunity. 2017;46:29–37.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  4. Arnold KB, et al. Increased levels of inflammatory cytokines in the female reproductive tract are associated with altered expression of proteases, mucosal barrier proteins, and an influx of HIV-susceptible target cells. Mucosal Immunol. 2016;9:194–205.

    Article  CAS  PubMed  Google Scholar 

  5. McKinnon LR, et al. Genital inflammation undermines the effectiveness of tenofovir gel in preventing HIV acquisition in women. Nat Med. 2018;24:491–6.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  6. Dabee S, Passmore JS, Heffron R, Jaspan HB. The Complex Link between the Female Genital Microbiota, Genital Infections, and Inflammation. Infect Immun. 2021;89:1–19.

  7. Sobia P, et al. Higher mucosal antibody concentrations in women with genital tract inflammation. Sci Rep. 2021;11:23514.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  8. Ilhan ZE, et al. Deciphering the complex interplay between microbiota, HPV, inflammation and cancer through cervicovaginal metabolic profiling. EBioMedicine. 2019;44:675–90.

    Article  PubMed  PubMed Central  Google Scholar 

  9. Laniewski P, et al. Features of the cervicovaginal microenvironment drive cancer biomarker signatures in patients across cervical carcinogenesis. Sci Rep. 2019;9:7333.

    Article  PubMed  PubMed Central  Google Scholar 

  10. Castle PE, et al. An association of cervical inflammation with high-grade cervical neoplasia in women infected with oncogenic human papillomavirus (HPV). Cancer Epidemiol Biomarkers Prev. 2001;10:1021–7.

    CAS  PubMed  Google Scholar 

  11. de Castro-Sobrinho JM, et al. Bacterial vaginosis and inflammatory response showed association with severity of cervical neoplasia in HPV-positive women. Diagn Cytopathol. 2016;44:80–6.

    Article  PubMed  Google Scholar 

  12. Chan D, et al. Microbial-driven preterm labour involves crosstalk between the innate and adaptive immune response. Nat Commun. 2022;13:975.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  13. Hezelgrave NL, et al. Cervicovaginal natural antimicrobial expression in pregnancy and association with spontaneous preterm birth. Sci Rep. 2020;10:12018.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  14. Fichorova RN, et al. Aberrant cervical innate immunity predicts onset of dysbiosis and sexually transmitted infections in women of reproductive age. PLoS One. 2020;15:e0224359.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  15. Simhan HN, Caritis SN, Krohn MA, Hillier SL. The vaginal inflammatory milieu and the risk of early premature preterm rupture of membranes. Am J Obstet Gynecol. 2005;192:213–8.

    Article  PubMed  Google Scholar 

  16. Barros MR Jr, et al. Activities of stromal and immune cells in HPV-related cancers. J Exp Clin Cancer Res. 2018;37:137.

    Article  PubMed  PubMed Central  Google Scholar 

  17. Punt S, et al. Angels and demons: Th17 cells represent a beneficial response, while neutrophil IL-17 is associated with poor prognosis in squamous cervical cancer. Oncoimmunology. 2015;4: e984539.

    Article  PubMed  PubMed Central  Google Scholar 

  18. Hibma MH. The immune response to papillomavirus during infection persistence and regression. Open Virol J. 2012;6:241–8.

    Article  PubMed  PubMed Central  Google Scholar 

  19. Kobayashi A, et al. Functional attributes of mucosal immunity in cervical intraepithelial neoplasia and effects of HIV infection. Cancer Res. 2004;64:6766–74.

    Article  CAS  PubMed  Google Scholar 

  20. Carus A, Ladekarl M, Hager H, Nedergaard BS, Donskov F. Tumour-associated CD66b+ neutrophil count is an independent prognostic factor for recurrence in localised cervical cancer. Br J Cancer. 2013;108:2116–22.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  21. Noel-Romas L, et al. Vaginal microbiome-hormonal contraceptive interactions associate with the mucosal proteome and HIV acquisition. PLoS Pathog. 2020;16:e1009097.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  22. Jespers V, et al. A longitudinal analysis of the vaginal microbiota and vaginal immune mediators in women from sub-Saharan Africa. Sci Rep. 2017;7:11974.

    Article  PubMed  PubMed Central  Google Scholar 

  23. Masson L, et al. Defining genital tract cytokine signatures of sexually transmitted infections and bacterial vaginosis in women at high risk of HIV infection: a cross-sectional study. Sex Transm Infect. 2014;90:580–7.

    Article  PubMed  Google Scholar 

  24. Lee SK, Kim CJ, Kim DJ, Kang JH. Immune cells in the female reproductive tract. Immune Netw. 2015;15:16–26.

    Article  PubMed  PubMed Central  Google Scholar 

  25. Wira CR, Rodriguez-Garcia M, Patel MV. The role of sex hormones in immune protection of the female reproductive tract. Nat Rev Immunol. 2015;15:217–30.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  26. Givan AL, et al. Flow cytometric analysis of leukocytes in the human female reproductive tract: comparison of fallopian tube, uterus, cervix, and vagina. Am J Reprod Immunol. 1997;38:350–9.

    Article  CAS  PubMed  Google Scholar 

  27. Anahtar MN, et al. Cervicovaginal bacteria are a major modulator of host inflammatory responses in the female genital tract. Immunity. 2015;42:965–76.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  28. Alisoltani A, et al. Microbial function and genital inflammation in young South African women at high risk of HIV infection. Microbiome. 2020;8:165.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  29. Ravel J, et al. Vaginal microbiome of reproductive-age women. Proc Natl Acad Sci U S A. 2011;108(Suppl 1):4680–7.

    Article  CAS  PubMed  Google Scholar 

  30. Kenyon CR, Osbak K. Recent progress in understanding the epidemiology of bacterial vaginosis. Curr Opin Obstet Gynecol. 2014;26:448–54.

    Article  PubMed  Google Scholar 

  31. L. R. McKinnon et al., The evolving facets of bacterial vaginosis: implications for HIV transmission. AIDS Res Hum Retroviruses. 2019.

  32. Peebles K, Velloza J, Balkus JE, McClelland RS, Barnabas RV. High global burden and costs of bacterial vaginosis: a systematic review and meta-analysis. Sex Transm Dis. 2019;46:304–11.

    Article  PubMed  Google Scholar 

  33. Bilardi JE, et al. The burden of bacterial vaginosis: women’s experience of the physical, emotional, sexual and social impact of living with recurrent bacterial vaginosis. PLoS One. 2013;8:e74378.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  34. Paladine HL, Desai UA. Vaginitis: diagnosis and treatment. Am Fam Physician. 2018;97:321–9.

    PubMed  Google Scholar 

  35. Anahtar MN, Gootenberg DB, Mitchell CM, Kwon DS. Cervicovaginal microbiota and reproductive health: the virtue of simplicity. Cell Host Microbe. 2018;23:159–68.

    Article  CAS  PubMed  Google Scholar 

  36. Aldunate M, et al. Antimicrobial and immune modulatory effects of lactic acid and short chain fatty acids produced by vaginal microbiota associated with eubiosis and bacterial vaginosis. Front Physiol. 2015;6:164.

    Article  PubMed  PubMed Central  Google Scholar 

  37. Shannon B, et al. Distinct effects of the cervicovaginal microbiota and herpes simplex type 2 infection on female genital tract immunology. J Infect Dis. 2017;215:1366–75.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  38. Mysorekar IU, Cao B. Microbiome in parturition and preterm birth. Semin Reprod Med. 2014;32:50–5.

    Article  CAS  PubMed  Google Scholar 

  39. Mitchell C, Marrazzo J. Bacterial vaginosis and the cervicovaginal immune response. Am J Reprod Immunol. 2014;71:555–63.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  40. Spear GT, et al. Multiplex immunoassay of lower genital tract mucosal fluid from women attending an urban STD clinic shows broadly increased IL1ß and lactoferrin. PLoS One. 2011;6:e19560.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  41. Cauci S, Driussi S, Guaschino S, Isola M, Quadrifoglio F. Correlation of local interleukin-1beta levels with specific IgA response against Gardnerella vaginalis cytolysin in women with bacterial vaginosis. Am J Reprod Immunol. 2002;47:257–64.

    Article  PubMed  Google Scholar 

  42. Balkus J, Agnew K, Lawler R, Mitchell C, Hitti J. Effects of pregnancy and bacterial vaginosis on proinflammatory cytokine and secretory leukocyte protease inhibitor concentrations in vaginal secretions. J Pregnancy. 2010;2010:385981.

    Article  PubMed  PubMed Central  Google Scholar 

  43. Santos-Greatti MMV, da Silva MG, Ferreira CST, Marconi C. Cervicovaginal cytokines, sialidase activity and bacterial load in reproductive-aged women with intermediate vaginal flora. J Reprod Immunol. 2016;118:36–41.

    Article  CAS  PubMed  Google Scholar 

  44. Hedges SR, Barrientes F, Desmond RA, Schwebke JR. Local and systemic cytokine levels in relation to changes in vaginal flora. J Infect Dis. 2006;193:556–62.

    Article  CAS  PubMed  Google Scholar 

  45. Muzny CA, Łaniewski P, Schwebke JR, Herbst-Kralovetz MM. Host-vaginal microbiota interactions in the pathogenesis of bacterial vaginosis. Curr Opin Infect Dis. 2020;33:59–65.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  46. Murphy K, Mitchell CM. The Interplay of Host Immunity, Environment and the Risk of Bacterial Vaginosis and Associated Reproductive Health Outcomes. J Infect Dis. 2016;214(Suppl 1):S29–35.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  47. Diaz-Cueto L, et al. Effect of clindamycin treatment on vaginal inflammatory markers in pregnant women with bacterial vaginosis and a positive fetal fibronectin test. Int J Gynaecol Obstet. 2009;107:143–6.

    Article  CAS  PubMed  Google Scholar 

  48. Alcaide ML, et al. High levels of inflammatory cytokines in the reproductive tract of women with BV and engaging in intravaginal douching: a cross-sectional study of participants in the women interagency HIV study. AIDS Res Hum Retroviruses. 2017;33:309–17.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  49. Campisciano G, Zanotta N, Licastro D, De Seta F, Comar M. In vivo microbiome and associated immune markers: new insights into the pathogenesis of vaginal dysbiosis. Sci Rep. 2018;8:2307.

    Article  PubMed  PubMed Central  Google Scholar 

  50. Chang PV, Hao L, Offermanns S, Medzhitov R. The microbial metabolite butyrate regulates intestinal macrophage function via histone deacetylase inhibition. Proc Natl Acad Sci U S A. 2014;111:2247–52.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  51. Arpaia N, Rudensky AY. Microbial metabolites control gut inflammatory responses. Proc Natl Acad Sci U S A. 2014;111:2058–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  52. Srinivasan S, et al. Metabolic signatures of bacterial vaginosis. mBio. 2015;6:1–16

  53. Borgogna JC, et al. Biogenic amines increase the odds of bacterial vaginosis and affect the growth of and lactic acid production by vaginal Lactobacillus spp. Appl Environ Microbiol. 2021;87:1–16.

  54. Yeoman CJ, et al. A multi-omic systems-based approach reveals metabolic markers of bacterial vaginosis and insight into the disease. PLoS One. 2013;8:e56111.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  55. Delgado-Diaz DJ, et al. Distinct immune responses elicited from cervicovaginal epithelial cells by lactic acid and short chain fatty acids associated with optimal and non-optimal vaginal microbiota. Front Cell Infect Microbiol. 2019;9:446.

    Article  CAS  PubMed  Google Scholar 

  56. Hearps AC, et al. Vaginal lactic acid elicits an anti-inflammatory response from human cervicovaginal epithelial cells and inhibits production of pro-inflammatory mediators associated with HIV acquisition. Mucosal Immunol. 2017;10:1480–90.

    Article  CAS  PubMed  Google Scholar 

  57. Amsel R, et al. Nonspecific vaginitis. Diagnostic criteria and microbial and epidemiologic associations. Am J Med. 1983;74:14–22.

    Article  CAS  PubMed  Google Scholar 

  58. Birse KM, et al. Unbiased proteomics analysis demonstrates significant variability in mucosal immune factor expression depending on the site and method of collection. PLoS One. 2013;8:e79505.

    Article  PubMed  PubMed Central  Google Scholar 

  59. Farr Zuend C, et al. Pregnancy associates with alterations to the host and microbial proteome in vaginal mucosa. Am J Reprod Immunol. 2020;83:e13235.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  60. Kamburov A, Wierling C, Lehrach H, Herwig R. ConsensusPathDB–a database for integrating human functional interaction networks. Nucleic Acids Res. 2009;37:D623–628.

    Article  CAS  PubMed  Google Scholar 

  61. Kamburov A, et al. ConsensusPathDB: toward a more complete picture of cell biology. Nucleic Acids Res. 2011;39:D712–717.

    Article  CAS  PubMed  Google Scholar 

  62. Kamburov A, Stelzl U, Lehrach H, Herwig R. The ConsensusPathDB interaction database: 2013 update. Nucleic Acids Res. 2013;41:D793–800.

    Article  CAS  PubMed  Google Scholar 

  63. Herwig R, Hardt C, Lienhard M, Kamburov A. Analyzing and interpreting genome data at the network level with ConsensusPathDB. Nat Protoc. 2016;11:1889–907.

    Article  CAS  PubMed  Google Scholar 

  64. Klatt NR, et al. Vaginal bacteria modify HIV tenofovir microbicide efficacy in African women. Science. 2017;356:938–45.

    Article  CAS  PubMed  Google Scholar 

  65. Kanehisa M, Sato Y, Morishima K. BlastKOALA and GhostKOALA: KEGG Tools for Functional Characterization of Genome and Metagenome Sequences. J Mol Biol. 2016;428:726–31.

    Article  CAS  PubMed  Google Scholar 

  66. Liaw A, Wiener M. Classification and Regression by randomForest. The Newsletter of the R Project. R News 2/3. 2002.

  67. Bayesian Network with Examples in R. (Chapman and Hall, Boca Raton, Scutari, M., Denis, J.).

  68. Byrne EH, et al. Antigen Presenting Cells Link the Female Genital Tract Microbiome to Mucosal Inflammation, With Hormonal Contraception as an Additional Modulator of Inflammatory Signatures. Front Cell Infect Microbiol. 2021;11:733619.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  69. Rubic T, et al. Triggering the succinate receptor GPR91 on dendritic cells enhances immunity. Nat Immunol. 2008;9:1261–9.

    Article  CAS  PubMed  Google Scholar 

  70. Tannahill GM, et al. Succinate is an inflammatory signal that induces IL-1beta through HIF-1alpha. Nature. 2013;496:238–42.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  71. Graham LS, Krass L, Zariffard MR, Spear GT, Mirmonsef P. Effects of succinic acid and other microbial fermentation products on HIV expression in macrophages. Biores Open Access. 2013;2:385–91.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  72. Singh N, et al. Is myometrial inflammation a cause or a consequence of term human labour? J Endocrinol. 2017;235:69–83.

    Article  CAS  PubMed  Google Scholar 

  73. Thomson AJ, et al. Leukocytes infiltrate the myometrium during human parturition: further evidence that labour is an inflammatory process. Hum Reprod. 1999;14:229–36.

    Article  CAS  PubMed  Google Scholar 

  74. Nold C, et al. Block of Granulocyte-Macrophage Colony-Stimulating Factor Prevents Inflammation-Induced Preterm Birth in a Mouse Model for Parturition. Reprod Sci. 2019;26:551–9.

    Article  CAS  PubMed  Google Scholar 

  75. Dubicke A, Ekman-Ordeberg G, Mazurek P, Miller L, Yellon SM. Density of stromal cells and macrophages associated with collagen remodeling in the human cervix in preterm and term birth. Reprod Sci. 2016;23:595–603.

    Article  CAS  PubMed  Google Scholar 

  76. Myers DA. The recruitment and activation of leukocytes into the immune cervix: further support that cervical remodeling involves an immune and inflammatory mechanism. Biol Reprod. 2012;87:107.

    Article  PubMed  Google Scholar 

  77. Lakomy DS, et al. Immune correlates of therapy outcomes in women with cervical cancer treated with chemoradiotherapy: A systematic review. Cancer Med. 2021;10:4206–20.

    Article  PubMed  PubMed Central  Google Scholar 

  78. Biswas SK, Allavena P, Mantovani A. Tumor-associated macrophages: functional diversity, clinical significance, and open questions. Semin Immunopathol. 2013;35:585–600.

    Article  CAS  PubMed  Google Scholar 

  79. Tang X, Mo C, Wang Y, Wei D, Xiao H. Anti-tumour strategies aiming to target tumour-associated macrophages. Immunology. 2013;138:93–104.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  80. Ding H, et al. Tumor-associated macrophages induce lymphangiogenesis in cervical cancer via interaction with tumor cells. APMIS. 2014;122:1059–69.

    CAS  PubMed  Google Scholar 

  81. Tett A, Pasolli E, Masetti G, Ercolini D, Segata N. Prevotella diversity, niches and interactions with the human host. Nat Rev Microbiol. 2021;19:585–99.

    Article  CAS  PubMed  Google Scholar 

  82. Dunlop AL, et al. Vaginal microbiome composition in early pregnancy and risk of spontaneous preterm and early term birth among African American women. Front Cell Infect Microbiol. 2021;11:641005.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  83. Tachedjian G, Aldunate M, Bradshaw CS, Cone RA. The role of lactic acid production by probiotic Lactobacillus species in vaginal health. Res Microbiol. 2017;168:782–92.

    Article  CAS  PubMed  Google Scholar 

  84. Manhanzva MT, et al. Inflammatory and antimicrobial properties differ between vaginal Lactobacillus isolates from South African women with non-optimal versus optimal microbiota. Sci Rep. 2020;10:6196.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  85. Wu SE, et al. Microbiota-derived metabolite promotes HDAC3 activity in the gut. Nature. 2020;586:108–12.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  86. Watson PJ, et al. Insights into the activation mechanism of class I HDAC complexes by inositol phosphates. Nat Commun. 2016;7:11262.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  87. Brown AG, Tulina NM, Barila GO, Hester MS, Elovitz MA. Exposure to intrauterine inflammation alters metabolomic profiles in the amniotic fluid, fetal and neonatal brain in the mouse. PLoS One. 2017;12:e0186656.

    Article  PubMed  PubMed Central  Google Scholar 

  88. Marangoni A, et al. New insights into vaginal environment during pregnancy. Front Mol Biosci. 2021;8:656844.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  89. Mager LF, et al. Microbiome-derived inosine modulates response to checkpoint inhibitor immunotherapy. Science. 2020;369:1481–9.

    Article  CAS  PubMed  Google Scholar 

  90. Wang T, et al. Inosine is an alternative carbon source for CD8(+)-T-cell function under glucose restriction. Nat Metab. 2020;2:635–47.

    Article  PubMed  PubMed Central  Google Scholar 

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We thank Max Abou for technical assistance.


Funding for this study was provided by the Canadian Institutes of Health Research Innovative Biomedical and Clinical HIV/AIDS Research: Team grant (ADB, VP: HB3-164066)

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Authors and Affiliations



ADB and VP conceived the study. CFZ, AL, KB, KK, PM, MP, HA, JJS, FS, JJS, ARB, SM, and GW performed the experimental analysis of specimens and generated data. CFZ, AL, LNR, SK, and SM performed analysis and interpreted the data. FM, BS, AY, MB, ARB, and VP managed the study cohort. CFZ, AL, and ADB wrote the manuscript.

Corresponding authors

Correspondence to Christina Farr Zuend or Adam D. Burgener.

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Ethics approval and consent to participate

This study was approved by the Research Ethics Board at the University of Manitoba (Study: HS20497). Written informed consent was obtained from all study participants.

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Not applicable.

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The authors declare that they have no competing interests.

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Supplementary Information

Additional file 1: Supplemental Table 1.

Metabolites that differ by inflammation status or Lactobacillus dominance.

Additional file 2: Supplemental Figure 1.

Representative overview of gating strategy. CMCs were dislodged from cytobrushes and stained with an optimized antibody cocktail to identify immune cell lineages. Data was acquired on an LSRII (BD Biosciences) and analyzed using FlowJo. Forward and side scatter were used to identify cells, and then singlets were gated. A fixable viability dye was used to identify live cells and then cells were gated based on expression of CD3. CD3+ cells were gated to determine expression of CD4 and CD8. CD3- cells were examined for expression of CD19 and CD56. CD19-CD56- cells were examined for expression of CD14. CD14- cells were examined for expression of CD15 and CD16, then CD49d expression on CD15+CD16+ was examined. PBMCs were used for instrument set up and gating including unstained PBMCs, single colour controls, and FMOs.

Additional file 3.


Additional file 4. 

Proteomics results_batch 1.

Additional file 5.

 Proteomics results_batch 2.

Additional file 6.

 Metaproteome results.

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Farr Zuend, C., Lamont, A., Noel-Romas, L. et al. Increased genital mucosal cytokines in Canadian women associate with higher antigen-presenting cells, inflammatory metabolites, epithelial barrier disruption, and the depletion of L. crispatus. Microbiome 11, 159 (2023).

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  • Inflammation
  • Antigen-presenting cells
  • Microbiome
  • Metaproteome
  • Metabolome