Depletion of dietary aryl hydrocarbon receptor ligands alters microbiota composition and function

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Abstract

The intestinal microbiota is critical for maintaining homeostasis. Dysbiosis, an imbalance in the microbial community, contributes to the susceptibility of several diseases. Many factors are known to influence gut microbial composition, including diet. We have previously shown that fecal immunoglobulin (Ig) A levels are decreased in mice fed a diet free of aryl hydrocarbon receptor (AhR) ligands. Here, we hypothesize this IgA decrease is secondary to diet-induced dysbiosis. We assigned mice to a conventional diet, an AhR ligand-free diet, or an AhR ligand-free diet supplemented with the dietary AhR ligand indole-3-carbinol (I3C). We observed a global alteration of fecal microbiota upon dietary AhR ligand deprivation. Compared to mice on the conventional diet, family Erysipelotrichaceae was enriched in the feces of mice on the AhR ligand-free diet but returned to normal levels upon dietary supplementation with I3C. Faecalibaculum rodentium, an Erysipelotrichaceae species, depleted its growth media of AhR ligands. Cultured fecal bacteria from mice on the AhR ligand-free diet, but not the other two diets, were able to alter IgA levels in vitro, as was F. rodentium alone. Our data point to the critical role of AhR dietary ligands in shaping the composition and proper functioning of gut microbiota.

Introduction

The aryl hydrocarbon receptor (AhR) is a transcription factor that was originally studied for its role in mediating the metabolism of its xenobiotic ligands. As a sensor of environmental chemicals, AhR is heavily expressed at barrier sites such as the skin, lungs, and gut1. More recently, physiological AhR ligands have been identified, including gut microbiota-derived tryptophan metabolites2,3,4 and dietary compounds5. A growing body of work illustrates the vital role of AhR in maintaining gut health and homeostasis. AhR antagonism leads to more severe chemically-induced colitis, and expression of AhR is reduced in intestinal tissue of ulcerative colitis (UC) patients6. The serum level of indole-3-propionic acid (IPA), an AhR ligand generated from microbial tryptophan catabolism, is decreased in both UC patients and in experimental murine colitis. Importantly, oral administration of IPA to mice ameliorated disease7. Mice deficient in caspase recruitment domain 9 (Card9), an inflammatory bowel disease (IBD) susceptibility gene, harbor a dysbiotic gut microbiota that is unable to metabolize tryptophan into AhR ligands, leading to more severe chemically-induced colitis8. Dietary sources of AhR ligands that are not directly produced by the microbiota are also capable of modulating the gut environment. Perhaps one of the best studied dietary sources of AhR ligands is indole-3-carbinol (I3C), which upon ingestion is converted by acid hydrolysis in the stomach to high-affinity AhR ligands such as indolo[3,2-b]carbazole (ICZ)9,10 and 3,3′-diindolylmethane (DIM)11. Dietary supplementation with I3C protects mice from developing colorectal cancer and ameliorates tumorigenesis already in progress12. In addition, mice on a diet low in AhR ligands harbor a higher gut bacterial load compared with mice on a control diet, and dietary I3C is sufficient to lower the bacterial load to normal levels13.

We have shown previously that mice fed a diet deficient in AhR ligands have lower levels of fecal immunoglobulin (Ig) A compared with mice on a conventional chow diet14. IgA is the predominant antibody isotype at mucosal sites, and throughout the body, more IgA is produced than every other antibody isotype combined15. Although it has long been known that IgA protects against infection from clear gastrointestinal pathogens such as Salmonella typhimurium16, Vibrio cholera17 and Shigella flexneri18, IgA coating of commensal microbes in human19 and mouse20 fecal samples has been described. Mouse experiments have indicated that proper IgA coating of gut commensals requires functional B cell selection and affinity maturation21, suggesting IgA coating of commensal microbes is largely a specific response rather than a product of cross-reactivity. In patients with IBD, the percentage of fecal microbes bound by IgA increases22. Because dysbiosis is a hallmark of IBD23, it has been speculated that IgA particularly targets pathobionts24, members of the microbiota with the potential to directly stimulate a potent inflammatory response. Coating of gut microbiota with IgA does not seem to inhibit bacterial growth or cause clearance, but is considered vital for proper physical containment of the microbes and for immune homeostasis25,26. Therefore, a deficiency in gut IgA for any reason, even in the absence of overt pathogens, can result in deleterious consequences for gastrointestinal health27.

Previous studies have demonstrated that certain pathogenic bacterial species28,29 as well as whole fecal microbiota from mice30 have the ability to degrade IgA. Here, we hypothesized that an AhR ligand-free diet would alter the composition of the microbiota, and that this altered microbiota directly contributes to the low fecal IgA levels characteristic of mice on this diet. We also sought to identify potential commensal species capable of shaping luminal IgA levels.

Methods

Animal husbandry and special diets

C57BL/6 mice were purchased from Jackson Laboratories (Bar Harbor, ME) and bred in our animal facility to obtain the mice used in this study. Special diets were created and administered as previously described14. In brief, the AhR ligand-free diet AIN-76A and AIN-76A supplemented with indole-3-carbinol (1000 parts per million)31 were purchased from Envigo. Mice were placed on their respective diets immediately after weaning, at approximately 2 weeks of age, and fecal samples were collected 8 weeks later. Animals were bred and maintained under specific pathogen-free conditions in Thoren Isolator racks under positive pressure. All experiments involving animals were approved by the Institutional Animal Care and Use Committee at the University of Alabama at Birmingham.

16S rDNA sequencing and bioinformatics analysis

DNA was isolated from fecal pellets using the ZR Fecal DNA MiniPrep Kit (Zymo Research, Irvine, CA, USA). PCR, sequencing, and bioinformatics analysis were performed as we have described previously32.

A BLAST analysis (National Center for Biotechnology Information) was performed on all of the Erysipelotrichaceae 16S rDNA sequences that were among the top 100 most abundant operational taxonomic units (OTUs) from each group of mice in the study. Sequences were searched against the 16S ribosomal RNA database and optimized for a megablast algorithm. Results are valid as of June 7, 2018.

Culturing of fecal microbes

Fresh fecal samples from four mice on a conventional diet were pooled, fecal samples from three mice on the AhR ligand-free diet were pooled, and fecal samples from three mice on the AhR ligand-free diet supplemented with I3C were pooled. These pooled samples were weighed and resuspended in sterile PBS to a concentration of 200 mg/mL. Chopped meat carbohydrate broth (BD Biosciences, San Jose, CA, USA) was inoculated with 250 µl of this suspension and cultured at 37 °C overnight in an anaerobic chamber. The following day, cultures were aliquoted and stored at −80 °C until being used in IgA transcytosis and luciferase assays described below.

Bacterial culture and preparation of bead-beaten extracts

Faecalibaculum rodentium strain ALO17 was purchased from Deutsche Sammlung von Mikroorganismen und Zellkulturen (DSMZ) (Braunschweig, Germany). Frozen isolates of F. rodentium were swabbed on a blood agar plate and incubated at 37 °C in an anaerobic chamber (day 0). On day 5, a single colony on the plate was transferred into a vial of chopped meat broth with carbohydrates (BD). After an additional 2 days, 1 mL of bacteria-containing broth was transferred to 2 tubes each of chopped meat broth with carbohydrates and 2 tubes each of chopped meat broth with no carbohydrates (Anaerobe Systems, Morgan Hill, CA, USA). L-Tryptophan (Sigma, St. Louis, MO, USA) was dissolved in PBS to create a 70 mM solution. Hydrochloric acid was added dropwise until tryptophan was fully dissolved. After the solution was sterile filtered, an appropriate volume was added to 1 tube of bacteria in chopped meat with carbohydrates and 1 tube of bacteria in chopped meat with no carbohydrates to achieve a tryptophan concentration of 0.6 mM. Therefore, four culture conditions were created: 1) F. rodentium in chopped meat broth with carbohydrates 2) F. rodentium in chopped meat broth with carbohydrates and exogenous tryptophan 3) F. rodentium in chopped meat broth with no carbohydrates 4) F. rodentium in chopped meat broth with no carbohydrates but with exogenous tryptophan. After a final 24-hour incubation, the optical density of each culture at 600 nm (OD600) was measured (0.759, 0.937, 0.468, and 0.474, respectively). After this measurement, broth samples were transferred to a 15 mL tube, centrifuged for 20 minutes at 3000 RPM, and supernatants collected and frozen at −80 °C until needed. To prepare bead-beaten extracts, the pellets were re-suspended in 500ul of PBS and transferred to 2 mL microcentrifuge tubes fitted with a rubber seal. BioSpec 0.1 mm glass beads (Fisher Scientific) were added to the tubes and tubes were beaten in a Mini Bead-Beater (Biospec Products, Bartlesville, OK, USA) for 1 minute. After beating, tubes were centrifuged at 13,000 RPM for 2 minutes and the extracts were collected. The amount of total protein in the extracts was quantified by the DC Protein Assay (Bio-Rad, Hercules, CA, USA). Extracts were stored at −80 °C until needed.

Lactobacillus reuteri strain PTA-6475 was purchased from American Type Culture Collection (ATCC) (Manassas, VA, USA). Frozen isolates were plated on a MRS agar plate and incubated in an anaerobic chamber at 37 °C for 48 hours. After this incubation, a single colony on the plate was inoculated into MRS broth and allowed to incubate for an additional 24 hours. The next day, the bacteria-containing broth was diluted 1:10 into 2 vials of fresh MRS broth and 2 vials of fresh carbohydrate-free peptone-tryptone water (Sigma). A volume of the tryptophan solution described above was added to 1 vial of MRS broth and 1 vial of peptone-tryptone water to achieve a tryptophan concentration of 0.6 mM. After a final 24-hour incubation, the vials were centrifuged and supernatants collected and frozen at −80 °C until needed.

AhR ligand luciferase reporter assay

HCT116 cells that have been engineered to express luciferase under the control of the dioxin response element were kindly provided by Dr. Greg Kennedy at the University of Alabama at Birmingham and were seeded in 96-well white wall plates (Corning, Corning, NY, USA) at a density of 10,000 cells per well. Cells were cultured in Dulbecco’s modified Eagle’s Medium (DMEM) supplemented with 10% fetal bovine serum (FBS), 100 U/mL of penicillin, 100 µg/mL of streptomycin, nonessential amino acids, 2 mM L-glutamine, and 100 µg/mL of hygromycin, all from Gibco except for hygromycin (Invitrogen, Carlsbad, CA, USA). The next day, cells were treated with bacteria-conditioned or non-conditioned broth at a dilution of 1:8 by volume or with 50 µg or 100 µg total protein of F. rodentium extract. As a positive control, some cells were treated with 100 nM of 6-formylindolo[3,2-b]carbazole (FICZ, purchased from Sigma), a known AhR ligand. Dimethyl sulfoxide (DMSO), the FICZ vehicle, was used as the negative control. After a 6 hour incubation at 37 °C, supernatants were discarded and cells were rinsed with PBS. Cells were subsequently lysed and treated with luciferase substrate using the Luciferase Assay System (Promega, Madison, WI, USA). Light intensity was measured with a SpectaMax L luminometer (Molecular Devices, San Jose, CA, USA) and data collected with Softmax version 5.4.5 software (Molecular Devices).

Colonic spheroid and transwell monolayer culture

Primary colonic epithelial stem cells were isolated, grown, and maintained as spheroids as previously described30,33. Briefly, mouse colon was harvested, washed with PBS, minced, and digested in a 2 mg/mL solution of collagenase type 1 (Gibco) for 50 minutes at 37 °C. Minced tissue in this solution was then filtered through a 70 µm cell strainer and filtered cells were centrifuged at 930 RPM for 5 minutes. Pelleted cells were then resuspended in Matrigel (BD Biosciences), plated onto a 24-well plate, and cultured in 50% L-WRN (L cells expressing Wnt3a, R-spondin3, and Noggin) conditioned medium. The L-WRN medium was supplemented with 10 µM of the Rho-associated protein kinase (ROCK) inhibitor Y27632 and 10 µM of the transforming growth factor (TGF)-β type I receptor inhibitor SB431542, both from R&D Systems (Minneapolis, MN, USA). L-WRN medium was replaced every 2 days, and spheroids were passaged every 3 days.

Epithelial cell monolayers from these spheroids were generated as previously described34. Briefly, 3-day-old spheroids were washed in a solution of 0.5 mM EDTA in PBS, dissociated into single cells by incubation in 0.05% trypsin/0.5 mM EDTA solution (Gibco) for 3.5 minutes at 37 °C, washed in DMEM/F12 media (Sigma) containing 10% FBS (Atlanta Biologicals, Flowery Branch, GA, USA), and filtered through a 40 µm cell strainer. Pelleted cells were then resuspended in 5% L-WRN conditioned medium supplemented with 10 µM Y27632 inhibitor and counted. 50% L-WRN medium was diluted to 5% using Advanced DMEM/F12 (Gibco) supplemented with 20% FBS (Atlanta Biologicals), 100 U/mL of penicillin, 100 µg/mL of streptomycin, and 2 mM L-glutamine. Transwell inserts (Corning) were coated with Matrigel diluted 1:30 in PBS. After incubation at 37 °C for 20–30 minutes, the Matrigel/PBS solution was removed and the cells immediately seeded in the apical Transwell compartment at a density of 100,000 cells per insert. This was considered day 0.

Cell treatments and IgA transcytosis assay

Cells in Transwell inserts were given fresh 5% L-WRN medium supplemented with 1 µg/mL lipopolysaccharide (LPS) (Sigma), 10 µM DAPT γ-secretase inhibitor (Millipore, Burlington, MA, USA), and 10 µM Y27632 inhibitor on days 1 and 2 of the monolayer culture.

IgA transcytosis assays were performed on day 3, as previously described30. Briefly, monolayers were removed from their treatment conditions and switched to fresh 5% L-WRN medium with 10 µM Y27632 inhibitor. 5 µg/mL IgA (BD Pharmingen) was added to the lower compartment. In the upper compartment, treatments included F. rodentium bead-beaten extract, supernatant conditioned by F. rodentium, or fecal bacteria cultures (all diluted 1:10 by volume). The extracts and conditioned supernatants derived from F. rodentium that were used for these experiments were generated from F. rodentium that had been grown in chopped meat broth with carbohydrates and no exogenous tryptophan. After incubating for 6 hours at 37 °C, apical supernatants were removed for IgA ELISA, cells in the Transwell were washed, transepithelial electrical resistance (TER) was measured, and RNA was collected from the cells (described below).

TER measurements

TER was measured from monolayers growing in Transwell inserts using an epithelial volt-ohm meter (World Precision Instruments, Sarasota, FL, USA). Two measurements were recorded. An initial measurement was taken on day 3 immediately before the addition of bacterial samples and IgA to the top and bottom compartments, respectively. Immediately after the 6 hour incubation allowed for the transcytosis assay, a second TER measurement was taken. The background TER measured from medium in a Transwell with no cells was subtracted from the resistance measured from a Transwell containing cells and medium. Each Transwell was measured in triplicate and the average value recorded.

Enzyme-linked immunosorbent assay

IgA levels in apical supernatants and mouse fecal samples were measured by ELISA, as we have previously described14.

Gene expression analysis

Immediately following collection of apical supernatants and the second TER measurement on day 3, cells in Transwell inserts were lysed in TRIzol Reagent (Invitrogen) and RNA was isolated according to the manufacturer’s instructions. Complementary DNA synthesis was performed using 200 ng of RNA and the High Capacity cDNA Reverse Transcription Kit (Applied Biosystems, Foster City, CA, USA). Quantitative polymerase chain reactions were performed with TaqMan Fast Advanced Master Mix (Applied Biosystems). Both reverse transcription and qPCR were performed in a QuantStudio 3 thermal cycler (ThermoFisher, Waltham, MA, USA). Expression levels for each sample were determined in duplicate and normalized to expression of glyceraldehyde 3-phosphate dehydrogenase (Gapdh) by the ΔΔCT method. The primers used were: Gapdh, assay ID Mm99999915_g1; and Pigr, assay ID Mm00465049_m1, both from ThermoFisher.

Metabolomics analysis

Metabolite extractions from media

100uL culture supernatant or non-conditioned chopped meat broth was added to 600 µL of acetonitrile to a Phree column (Phenomenex, Torrence CA) to remove intact protein and phospholipid content. The vacuum manifold extracted supernatant was then removed and dried under N2 gas. 100 µL of 0.1% Formic Acid was added to ddH20 for mass spectrometry evaluations.

NanocHiPLC-tandem mass spectrometry

An aliquot (5 µL) of each digest was loaded onto a Nano cHiPLC 200 µm × 6 mm ChromXP C18-CL 3 µm 120 Å reverse-phase trap cartridge (Eksigent, Toronto, Canada) at 2 µL/min using an Eksigent autosampler. After washing the cartridge for 5 min with 0.1% formic acid in ddH20, the bound peptides were flushed onto a Nano cHiPLC column 200 µm × 15 cm ChromXP C18-CL 3 µm 120 Å (Eksigent, Toronto, Canada) with a 20 min linear (2–98%) acetonitrile gradient in 0.1% formic acid at 1000 nl/min using an Eksigent 400 NanoLC System. (Dublin, CA). The column was washed with 98% acetonitrile-0.1% formic acid for 5 min and then re-equilibrated with 2% acetonitrile-0.1% formic acid for 5 min. The SCIEX 5600 Triple-Tof mass spectrometer (SCIEX, Toronto, Canada) was used to analyze the protein digest. The IonSpray voltage was 2300 V and the declustering potential was 80 V. Ionspray and curtain gases were set at 10 psi and 25 psi, respectively. The interface heater temperature was 120 °C. Eluted metabolites were subjected to a time-of-flight 250msec survey scan from 50–1000 m/z to determine the top twenty most intense ions for MSMS analysis. Product ion time-of-flight scans at 50 msec were carried out to obtain the tandem mass spectra of the selected parent ions over the range from m/z 50–1000 using a rolling collision energy parameter to determine the best fragmentation energies per compound mass.

Processing data to XCMS online and metaboanalyst software

LC-MS data were processed using XCMS-Online (https://xcmsonline.scripps.edu/) to identify and align peaks occurring across all samples. The data was then exported into individual Excel.csv files for each sample containing the m/z, peak area and retention time of each metabolite ion. The exported files were then organized and uploaded to MetaboAnalyst version 3.5 (http://www.metaboanalyst.ca/) for statistical evaluations.

Statistical analysis

Unless otherwise indicated, statistical significance between two groups was determined by two-tailed unpaired Student’s t test. Comparison of more than two groups was performed with one-way ANOVA followed by Tukey’s multiple comparisons test. Calculations were performed using GraphPad Prism software version 7.03. A P value of <0.05 was considered statistically significant.

Results

Fecal microbiota composition is altered is the absence of dietary AhR ligands

We have previously shown that mice fed an AhR ligand-free diet contain less fecal IgA than mice fed a conventional diet14. The reduction in fecal IgA in mice on the ligand-free diet led us to hypothesize that mice on this diet harbor a microbiota distinct from mice on a normal chow diet. Microbiota differences were confirmed by subjecting bacterial DNA in fecal samples to 16S rDNA gene sequencing. Weighted UniFrac distance analysis was employed. This distance measure takes into account the relative abundance of OTUs in a sample and accounts for evolutionary relatedness of OTUs in calculating the degree of similarity among samples. As seen in Fig. 1a, this analysis clearly shows a high degree of dissimilarity in the microbiota composition between mice on the conventional and AhR ligand-free diets. In addition, mice on the ligand-free diet on average possessed a less diverse microbiota compared to mice on a conventional diet, as revealed by the Shannon diversity index (Fig. 1b). The Shannon index is a measure of alpha diversity. A diversity score is calculated based on the number of OTUs (richness) in a sample and how evenly the relative abundance of the OTUs is distributed within a sample. The higher the richness and more even the distribution, the higher the alpha diversity score. Dietary supplementation of the known AhR dietary ligand I3C into the ligand-free diet altered global microbiota composition (Fig. 1a) but not intra-sample diversity (Fig. 1b) relative to mice on the AhR ligand-free diet.

Figure 1
figure1

Fecal microbiota composition is altered in the absence of dietary AhR ligands. (a) Weighted UniFrac analysis of the global fecal microbiota composition from mice on a conventional diet (n = 12), mice on the AhR ligand-free (LF) diet (n = 7), and mice on the AhR LF diet supplemented with I3C (AhR LF + I3C diet) (n = 6). Each dot represents one mouse. Comparisons between any two given groups show the significance of the overall microbiota difference. Differences in overall microbiota composition among groups were calculated by a PERMANOVA test using Quantitative Insights into Microbial Ecology software. (b) Alpha diversity analysis of the fecal microbiota (Shannon index). (c) Average proportion of the major phyla present in fecal samples from mice on the indicated diet. (d) Relative abundance of Erysipelotrichaceae. Error bars represent mean ± SEM. Data for a-d are pooled from two independent experiments. **p < 0.01 ****p < 0.0001, one-way ANOVA with Tukey’s multiple comparisons test.

We next sought to identify specific taxa that might be contributing to the global microbiota changes described above. We limited our search to taxa that met the following criteria: (1) The relative abundance is significantly altered in the AhR ligand-free diet group relative to the conventional diet group, (2) The relative abundance in the conventional diet group and AhR ligand-free + I3C diet group is similar, and (3) The relative abundance is at least 1% in all three groups. At the phylum level, the only taxon to meet all three criteria was Actinobacteria (Fig. 1c and Supplementary Fig. 1a). We next generated a table of all families represented in this study (Supplementary Table 1). Of these 44 families, only Erysipelotrichaceae and Bifidobacteriaceae met our criteria, with the relative abundance of both taxa increasing in the AhR ligand-free diet group relative to the conventional diet group and decreasing to similar levels as the conventional diet group upon supplementation of the AhR ligand-free diet with I3C (Fig. 1d and Supplementary Fig. 1b). Because the relative abundance of Erysipelotrichaceae in all 3 diet groups was substantially higher than Bifidobacteriaceae, and given the previously reported connection between Erysipelotrichaceae and AhR35, we chose to focus on Erysipelotrichaceae rather than Bifidobacteriaceae for the remainder of this study.

Faecalibaculum rodentium, an Erysipelotrichaceae species, consumes AhR ligands

The results above suggest either that Erysipelotrichaceae species favor an environment in which AhR is inactive (and thus the expansion when AhR is not activated by dietary ligands), or that the increase in Erysipelotrichaceae relative abundance on the AhR ligand free diet is a compensatory mechanism to generate Erysipelotrichaceae-derived AhR ligands when dietary AhR ligands are withheld. In order to perform functional studies to test these opposing hypotheses, we sought to identify an Erysipelotrichaceae species from our samples by performing a Basic Local Alignment Search Tool (BLAST) analysis on all of the Erysipelotrichaceae 16S rDNA sequences that were among the 100 most abundant OTUs in each of the three groups of mice (Supplementary Tables 25). In a combined dataset of all three groups (Supplementary Table 2) and for the conventional diet (Supplementary Table 3) and AhR ligand-free diet (Supplementary Table 4) groups, Erysipelotrichaceae was the most abundant OTU, while it was the second most abundant in the AhR ligand-free + I3C diet group (Supplementary Table 5). There were several more occurrences of this family in the top 100 OTU table for all groups, and in all cases BLAST analysis identified their 16S rDNA sequences as most closely matched to Faecalibaculum rodentium (Supplementary Tables 25). We therefore identified F. rodentium as a Erysipelotrichaceae species in our samples.

Members of the gut microbiota, such as Lactobacillus reuteri, have been shown to possess the ability to metabolize tryptophan into AhR ligands under carbohydrate-starvation conditions4. In order to determine if F. rodentium consumes or produces AhR ligands, we grew this bacterium under anaerobic conditions in chopped meat broth with or without carbohydrates and supplemented or not with exogenous tryptophan. We also cultured L. reuteri to serve as a positive control. After 24 hours of exogenous tryptophan treatment, we collected the bacteria-conditioned supernatants and prepared bead-beaten extracts. To measure the amount of AhR ligands present in these samples, we employed HCT116 cells with the luciferase gene under the control of a dioxin response element, allowing these cells to express luciferase upon AhR ligation and translocation to the nucleus. By treating this cell line with bacteria-conditioned supernatants or extracts, we were able to determine the relative levels of AhR ligands in the samples. We also treated our luciferase reporter cell line with broth that had not been conditioned with bacteria but that had been supplemented or not with exogenous tryptophan. Strikingly, the amount of AhR ligands in non-conditioned broth was significantly higher than in the corresponding F. rodentium-conditioned supernatant in all treatment groups (Fig. 2a).

Figure 2
figure2

Faecalibaculum rodentium, an Erysipelotrichaceae species, consumes AhR ligands. (a) HCT116 cells engineered to express luciferase upon AhR ligation were treated with bacterial conditioned supernatants from F. rodentium under the indicated conditions. Cells were also treated with non-conditioned broth to establish baseline levels of any AhR ligands present. As a positive control, some cells were treated with 100 nM of 6-formylindolo[3,2-b]carbazole (FICZ), a known AhR ligand. Dimethyl sulfoxide (DMSO), the FICZ vehicle, was used as a negative control. (b) Peak levels of indole-3-propionic acid (IPA) in broth cultures of F. rodentium cultured in chopped meat broth with carbohydrates and no exogenous Trp. Non-conditioned broth (media) shown for comparison. (c) F. rodentium bead-beaten extracts (total protein amount indicated) failed to induce light production compared with the negative control, indicating a lack of AhR ligands. CHO, carbohydrates. Trp, tryptophan. For a, n = 9 per group. For b, data are representative of 3 experiments. For c, n = 6 per group. Error bars show mean ± SEM. *p < 0.05 **p < 0.01 ***p < 0.001 ****p < 0.0001, Student’s t test.

In order to verify these results, and identify specific AhR ligands consumed by F. rodentium, we performed a metabolomics analysis on F. rodentium-conditioned supernatants and non-conditioned broth. We found that the levels of indole-3-propionic acid (IPA), a known AhR ligand7, decreased following culturing of F. rodentium (Fig. 2b). This decrease likely explains the dampened AhR signaling F. rodentium-conditioned supernatant induced in our luciferase cell reporter assays compared to non-conditioned broth (Fig. 2a).

In contrast to F. rodentium, while L. reuteri-conditioned supernatant contained lower levels of AhR ligands than the corresponding non-conditioned broth with carbohydrates and with or without exogenous tryptophan (Supplementary Fig. 2), in carbohydrate-free conditions with exogenous tryptophan added, L. reuteri-conditioned supernatant contained nearly twice the amount of AhR ligands compared to its corresponding non-conditioned broth, consistent with previous reports4. However, this was also true of the carbohydrate-free, no exogenous tryptophan condition, suggesting either that sufficient levels of tryptophan were already present in the broth for L. reuteri to metabolize into AhR ligands, or that L. reuteri is capable of metabolizing non-tryptophan sources into AhR ligands during carbohydrate starvation conditions. Indeed, a tryptophan-independent mechanism of AhR ligand production by L. reuteri was recently described36. Interestingly, no AhR ligands were present in the F. rodentium extracts for any treatment group, as indicated by the lack of light production relative to the negative control (Fig. 2c), suggesting that F. rodentium metabolizes AhR ligands within 24 hours of uptake, the time period that bacteria were in their final treatment conditions. Taken together, these data support the hypothesis that F. rodentium favors an environment in which AhR is inactive and is capable of consuming AhR ligands to promote such an environment.

We finally determined if whole fecal microbiota from mice on the three diets differed in their ability to produce or consume AhR ligands. As expected, fecal culture supernatants from mice on the conventional and AhR ligand-free + I3C diets were able to increase AhR signaling relative to non-conditioned culture media (Supplementary Fig. 3). Given our findings discussed above of F. rodentium-conditioned supernatants failing to stimulate AhR activity to the same level as non-conditioned culture media (Fig. 2a), we hypothesized that supernatants from AhR ligand-free cultures would display a similar deficiency in the ability of activate AhR. Surprisingly, we found microbiota from AhR ligand-free diet mice was able to stimulate AhR signaling to a greater extent than microbiota from either of the other two diets (Supplementary Fig. 3). These results would suggest that removal of AhR ligands from the diet results in a compensatory expansion in members of the microbiota with the ability to generate AhR ligands.

Fecal microbiota from mice on an AhR ligand-free diet directly reduce secretory IgA levels

Having shown an association between altered microbiota composition and reduced fecal IgA levels in mice on the AhR ligand-free diet, we next sought to determine if a direct cause-and-effect relationship existed. To do so, we added fecal cultures obtained from mice on either the conventional, AhR ligand-free, or AhR ligand-free + I3C diets to the apical surface of primary colonic epithelial cell monolayers differentiated from epithelial stem cell spheroids in order to model IgA transcytosis34. During IgA transcytosis, polymeric IgA that is secreted by plasma cells in the lamina propria binds to the polymeric Ig receptor (pIgR) on the basolateral side of the epithelium37,38,39. The pIgA-pIgR complex is then endocytosed and transported across the cell to the apical surface40,41,42. Cellular enzymes cleave the receptor, releasing secretory IgA (SIgA) into the lumen. However, SIgA is still bound to the extracellular portion of pIgR, known as secretory component, which makes SIgA less susceptible to cleavage by bacterial proteases43. In our in vitro model, primary epithelial stem cells from cultured spheroids were seeded in a Transwell insert and allowed to form into epithelial cell monolayers. After treatment with (N-[N-(3,5-difluorophenacetyl-L-alanyl)]-S-phenylglycine t-butyl ester (DAPT) and lipopolysaccharide (LPS) to promote cell differentiation and pIgR expression, respectively, IgA was added to the basal compartment of the Transwell at the same time as the bacterial cultures were added to the apical compartment (Fig. 3a). Six hours later, apical supernatants were collected and analyzed for IgA concentration.

Figure 3
figure3

Fecal microbiota from mice on an AhR ligand-free diet directly reduce secretory IgA levels. (a) Stem cells were isolated from the epithelial crypts of a mouse colon, cultured as spheroids, dissociated into single cells, and differentiated into epithelial cell monolayers. 100,000 stem cells were seeded into the apical compartment of a Transwell insert on day 0 and treated on days 1 and 2 with 1 µg/mL of lipopolysaccharide (LPS) and 10 µM (N-[N-(3,5-difluorophenacetyl-L-alanyl)]-S-phenylglycine t-butyl ester (DAPT) to induce expression of pIgR and differentiate the cells, respectively. As a negative control, some cells were not treated with LPS and DAPT (untreated). On day 3, cells were removed from their treatments and placed in fresh medium. IgA was added to the basal compartment of the Transwell at a concentration of 5 µg/mL. At the same time, bacterial fecal cultures from mice on the conventional diet (CD culture), AhR ligand-free diet (LF culture), or AhR ligand-free diet supplemented with I3C (I3C culture) were added to the apical compartment at a 1/10 dilution. (b) Medium in the apical compartment was collected 6 hours later and IgA levels assessed by ELISA. (c) On day 3, transepithelial electrical resistance (TER) of monolayers was measured immediately before adding fecal bacterial cultures. A second TER measurement was obtained 6 hours later. The data show this second TER measurement expressed as a percentage of the initial TER measurement. (d) Immediately after collection of apical supernatants and final TER measurements, cells were lysed in Trizol reagent, and Pigr expression was quantified by qPCR. Fold change in Pigr expression is relative to the untreated group. D, DAPT. L, LPS. For b, n = 5–8 per group. For c, n = 3–5 per group. For d, n = 3–6 per group. Error bars show mean ± SEM. *p < 0.05 **p < 0.01, one-way ANOVA with Tukey’s multiple comparisons test.

As expected, higher concentrations of IgA were observed in the apical supernatants of monolayers that were treated with DAPT and LPS compared with monolayers that were left untreated (Fig. 3b). Addition of bacterial cultures from conventional diet mice did not significantly alter the IgA concentration compared with DAPT and LPS treatment alone, whereas addition of bacterial cultures from AhR ligand-free mice led to an apical IgA concentration comparable to that observed from untreated monolayers (Fig. 3b). Importantly, addition of AhR ligand-free + I3C cultures resulted in apical IgA concentrations that were intermediate between those seen upon addition of conventional diet and AhR ligand-free cultures (Fig. 3b). IgA transcytosis requires an intact monolayer. If the physical integrity of the monolayer is compromised, IgA can passively diffuse across the membrane of the Transwell insert rather than actively being transcytosed through the epithelial cells. Therefore, in order to rule out the possibility that our results could be explained by differential effects of the fecal cultures on monolayer integrity, we measured transepithelial electrical resistance (TER) immediately before the addition of fecal cultures, followed by a second TER measurement six hours later. We found no significant differences in TER for any of the fecal cultures (Fig. 3c). Furthermore, it is unlikely that the decrease in apical IgA concentration observed upon addition of AhR ligand-free cultures can be explained by a deficiency in IgA transcytosis, because expression of Pigr among all the groups treated with DAPT and LPS was similar (Fig. 3d). We also observed a trend of increased fecal IgA concentration from mice on the AhR ligand-free + I3C diet compared to mice on the AhR ligand-free diet, although this increase did not reach statistical significance (Supplementary Fig. 4).

F. rodentium secretes factors that modulate SIgA levels

Finally, we sought to determine if a causative relationship exists between our observation of increased fecal Erysipelotrichaceae relative abundance and decreased fecal IgA in mice on an AhR ligand-free diet compared with mice on a conventional diet. To do so, we added F. rodentium bead-beaten extracts or conditioned supernatant to the apical compartment in our in vitro IgA transcytosis model. Six hours later, apical supernatants were collected.

As expected, we observed a higher concentration of IgA in the apical supernatants of monolayers treated with DAPT and LPS compared with monolayers that were left untreated (Fig. 4a,b). Addition of F. rodentium-conditioned supernatant to monolayers treated with DAPT and LPS led to a significant decrease in apical IgA concentration to levels comparable to the apical concentration seen in untreated monolayers. (Fig. 4a). In contrast to F. rodentium-conditioned supernatant, addition of F. rodentium bead-beaten extracts had no effect on the levels of apical IgA (Fig. 4b), suggesting factors secreted by F. rodentium, rather than cellular contents, are responsible for the observed decrease in apical IgA. Importantly, the ability of F. rodentium supernatant to lower apical IgA levels cannot be attributed to differential effects on TER (Fig. 4c) or Pigr expression (Fig. 4d) relative to DAPT + LPS treatment alone.

Figure 4
figure4

F. rodentium secretes factors that modulate SIgA levels. Stem cell spheroids were cultured and differentiated into epithelial cell monolayers as described in Fig. 3a. On day 3, F. rodentium-conditioned supernatant (a) or bead-beaten extracts (b) were added to the apical compartment of a Transwell insert at a 1/10 dilution, and 5 µg/mL IgA was added to the basal compartment. Six hours later, apical supernatants were collected and IgA levels assessed by ELISA. (c) An initial and final TER measurement was obtained as described in Fig. 3c. (d) Immediately after collection of apical supernatants and final TER measurements, cells from (a) were lysed in Trizol reagent and Pigr expression was quantified by qPCR. Fold change in Pigr expression is relative to the untreated group. D, DAPT. L, LPS. sup, supernatant. Error bars show mean ± SEM. For a, n = 8–9 per group. For b, n = 3 per group. For c, n = 3–5 per group. For d, n = 3–4 per group. *p < 0.05, one-way ANOVA with Tukey’s multiple comparisons test.

One possible interpretation of the collective results of Figs 3 and 4 is that microbiota from mice on the AhR ligand-free diet, and F. rodentium specifically, have the ability to degrade IgA. We attempted to perform immunoblotting on the apical supernatants to possibly visualize fragmented IgA, but the high amount of protein in chopped meat broth prevented us from doing so.

Discussion

Here we report that a diet devoid of AhR ligands leads to a fundamentally reshaped fecal microbiota, including an increase in the relative abundance of the family Erysipelotrichaceae. Even though addition of a single AhR ligand, I3C, to the AhR ligand-free diet was insufficient to completely restore the global microbiota composition to that of mice on a conventional diet, it was nevertheless sufficient to lower Erysipelotrichaceae relative abundance to a level similar to that observed in mice on a conventional diet.

There are conflicting reports regarding the potential beneficial or harmful effects of this family in inflammatory gastrointestinal disease. Ileitis-associated increases in Erysipelotrichaceae abundance have been reported in mice infected with Toxoplasma gondii or Giardia muris44, and this family is also expanded in a murine model of tumor necrosis factor (TNF)-driven Crohn’s disease (CD)-like ileitis45. In contrast, lower Erysipelotrichaceae abundance in humans has been associated with new-onset CD46 and recurring CD47. Collectively, these discrepancies might partially be explained by inherent differences in the gut microbiota between mice and humans48 and differential effects exerted by individual Erysipelotrichaceae species. Compared to gastrointestinal inflammation, there is more agreement concerning the relationship between Erysipelotrichaceae and metabolic disorders. Specifically, Erysipelotrichaceae abundance is elevated in mouse models of diet-induced obesity49,50,51 and in obese individuals52. On the other hand, low abundance of Erysipelotrichaceae has been associated with an increased chance of developing type 1 diabetes in the non-obese diabetic mouse model53.

Interestingly, it has been reported that mice fed a diet supplemented with broccoli, a rich source of AhR ligands, harbor a reduced abundance of Erysipelotrichaceae35. Our results provide evidence for the inverse as well: that a diet depleted of AhR ligands leads to an expansion of this bacterial family.

Given the beneficial and harmful properties associated with Erysipelotrichaceae, we sought to clarify in our own model whether or not the observed increase in Erysipelotrichaceae in mice on the AhR ligand-free diet represented a potentially beneficial or harmful event. In order to so, we first identified F. rodentium as the species most closely related to the Erysipelotrichaceae 16S rDNA sequences from mice in all three diets. We found that F. rodentium depletes its growth medium of AhR ligands. Furthermore, addition of F. rodentium-conditioned medium to the apical epithelial surface in an in vitro model of IgA transcytosis results in a decrease in apical IgA concentration. Based on these findings, we speculate that an increase in F. rodentium abundance in the context of dietary AhR ligand deficiency would represent an adverse event to the health of the host. However, whole microbiota from mice on the AhR ligand-free diet were able to recapitulate the IgA-reducing, but not the AhR ligand consuming, effects of F. rodentium. Given the greater susceptibility of mice with low fecal IgA levels to chemically-induced colitis30,54, future work will determine if the AhR ligand-free diet makes mice more susceptible to DSS colitis and if the microbiota in general and F. rodentium in particular directly contribute to the higher susceptibility.

As an essential amino acid, tryptophan cannot be synthesized by the host but must come from the diet. In the gastrointestinal tract, tryptophan can be directly metabolized into AhR ligands by the gut microbiota4. These microbial-derived ligands consist largely of indole derivatives2,7. Fecal samples from germ-free mice are deficient for AhR ligands8, underscoring the essential contribution made by the microbiota in regulating AhR activity. However, despite the well-established connection between commensal bacteria AhR ligand production and AhR physiological function55, the effects of disrupted AhR signaling on the composition and function of the gut microbiota has been understudied. Many studies involving suppression of AhR activity involve knockout of Ahr. However, we elected to investigate the effect of deficient AhR activity on the microbiota by instead withholding dietary AhR ligands, which represents a more physiologically relevant situation in terms of translational research. Our results utilizing cultured fecal bacteria from mice on the conventional, AhR ligand-free, and AhR ligand-free + I3C diets in our in vitro model of IgA transcytosis provide evidence that the reshaped fecal microbiota upon withholding of dietary AhR ligands is capable of directly decreasing IgA levels in the intestinal lumen. We propose that the Erysipelotrichaceae species F. rodentium is a contributor to this effect, because of our results incorporating F. rodentium-conditioned supernatant in our in vitro IgA transcytosis model and the decrease in Erysipelotrichaceae following supplementation of the AhR ligand-free diet with I3C.

Given our previous finding of reduced B cell numbers in intestinal Peyer’s patches from mice on the AhR ligand-free diet14, we cannot rule out the possibility that a deficiency in B cell gut recruitment and/or function contributes to lower fecal IgA levels in mice with no dietary sources of AhR ligands. Potential mechanisms linking AhR activation to B cell secretion of IgA is a source of ongoing work in our laboratory.

Dietary sources of AhR ligands fall into two main categories: flavonoids and other phytochemicals and tryptophan derivatives. Flavonoids are polyphenolic compounds found in a variety of fruits, vegetables, and plant-derived beverages such as tea and wine5. On the other hand, indole molecules, including I3C, are tryptophan derivatives. I3C is a metabolite of glucosinolate glucobrassicin, a major component of cruciferous vegetables56. Importantly, I3C and its derivatives possess anti-inflammatory properties in the setting of experimental systemic lupus erythematosus57 and chemically-induced colitis58. Although in the present study we supplemented the AhR ligand-free diet with only I3C, it would be of interest to investigate the effects other AhR dietary ligands exert on the microbiota.

We readily acknowledge our study has limitations. We were unable to show a statistically significant effect of I3C, when added to the AhR ligand-free diet, on fecal IgA levels. A relatively low sample size and high variability likely contributed to this failure, but the tendency of I3C supplementation to raise fecal IgA levels is clearly present. In addition, most of the Erysipelotrichaceae DNA sequences were not a 100% match to F. rodentium, even though F. rodentium was the closest possible species-level match according to our BLAST analysis. Nevertheless, it is possible that no actual AhR ligand-consuming taxa are present in the microbiota of mice on the AhR ligand-free diet, even if F. rodentium itself does have this characteristic. Such a scenario would explain our discordant results from the luciferase cell reporter assay utilizing culture supernatants of F. rodentium alone versus fecal samples from mice on the AhR ligand-free diet.

In conclusion, our results point to dietary AhR ligands as key factors in shaping the composition of the gut microbiota. A diet deficient in AhR ligands leads to an altered microbial community capable of decreasing IgA levels, an event that potentially increases susceptibility to colitis. F. rodentium was identified as likely contributing to IgA level modulation. Our data indicate that a diet rich in I3C might promote intestinal health by maintaining proper gut IgA levels through regulation of F. rodentium abundance. To our knowledge, this is the first time a specific bacterial commensal species has been implicated in modulating levels of AhR ligands and fecal IgA.

Data Availability

All microbiota DNA sequences generated in this study have been deposited in the Sequence Read Archive under accession number PRJNA510099.

References

  1. 1.

    Stockinger, B., Di Meglio, P., Gialitakis, M. & Duarte, J. H. The aryl hydrocarbon receptor: multitasking in the immune system. Annu Rev Immunol 32, 403–432, https://doi.org/10.1146/annurev-immunol-032713-120245 (2014).

  2. 2.

    Hubbard, T. D. et al. Adaptation of the human aryl hydrocarbon receptor to sense microbiota-derived indoles. Sci Rep 5, 12689, https://doi.org/10.1038/srep12689 (2015).

  3. 3.

    Lamas, B., Natividad, J. M. & Sokol, H. Aryl hydrocarbon receptor and intestinal immunity. Mucosal Immunol 11, 1024–1038, https://doi.org/10.1038/s41385-018-0019-2 (2018).

  4. 4.

    Zelante, T. et al. Tryptophan catabolites from microbiota engage aryl hydrocarbon receptor and balance mucosal reactivity via interleukin-22. Immunity 39, 372–385, https://doi.org/10.1016/j.immuni.2013.08.003 (2013).

  5. 5.

    Busbee, P. B., Rouse, M., Nagarkatti, M. & Nagarkatti, P. S. Use of natural AhR ligands as potential therapeutic modalities against inflammatory disorders. Nutr Rev 71, 353–369, https://doi.org/10.1111/nure.12024 (2013).

  6. 6.

    Monteleone, I. et al. Aryl hydrocarbon receptor-induced signals up-regulate IL-22 production and inhibit inflammation in the gastrointestinal tract. Gastroenterology 141(237–248), 248 e231, https://doi.org/10.1053/j.gastro.2011.04.007 (2011).

  7. 7.

    Alexeev, E. E. et al. Microbiota-Derived Indole Metabolites Promote Human and Murine Intestinal Homeostasis through Regulation of Interleukin-10 Receptor. Am J Pathol 188, 1183–1194, https://doi.org/10.1016/j.ajpath.2018.01.011 (2018).

  8. 8.

    Lamas, B. et al. CARD9 impacts colitis by altering gut microbiota metabolism of tryptophan into aryl hydrocarbon receptor ligands. Nat Med 22, 598–605, https://doi.org/10.1038/nm.4102 (2016).

  9. 9.

    Bjeldanes, L. F., Kim, J. Y., Grose, K. R., Bartholomew, J. C. & Bradfield, C. A. Aromatic hydrocarbon responsiveness-receptor agonists generated from indole-3-carbinol in vitro and in vivo: comparisons with 2,3,7,8-tetrachlorodibenzo-p-dioxin. Proc Natl Acad Sci USA 88, 9543–9547, https://doi.org/10.1073/pnas.88.21.9543 (1991).

  10. 10.

    Kleman, M. I., Poellinger, L. & Gustafsson, J. A. Regulation of human dioxin receptor function by indolocarbazoles, receptor ligands of dietary origin. J Biol Chem 269, 5137–5144 (1994).

  11. 11.

    Anderton, M. J. et al. Pharmacokinetics and tissue disposition of indole-3-carbinol and its acid condensation products after oral administration to mice. Clin Cancer Res 10, 5233–5241, https://doi.org/10.1158/1078-0432.CCR-04-0163 (2004).

  12. 12.

    Metidji, A. et al. The Environmental Sensor AHR Protects from Inflammatory Damage by Maintaining Intestinal Stem Cell Homeostasis and Barrier Integrity. Immunity 49, 353–362 e355, https://doi.org/10.1016/j.immuni.2018.07.010 (2018).

  13. 13.

    Li, Y. et al. Exogenous stimuli maintain intraepithelial lymphocytes via aryl hydrocarbon receptor activation. Cell 147, 629–640, https://doi.org/10.1016/j.cell.2011.09.025 (2011).

  14. 14.

    Culbreath, C. et al. Environmental-mediated intestinal homeostasis in neonatal mice. J Surg Res 198, 494–501, https://doi.org/10.1016/j.jss.2015.04.002 (2015).

  15. 15.

    Corthesy, B. Multi-faceted functions of secretory IgA at mucosal surfaces. Front Immunol 4, 185, https://doi.org/10.3389/fimmu.2013.00185 (2013).

  16. 16.

    Iankov, I. D. et al. Protective efficacy of IgA monoclonal antibodies to O and H antigens in a mouse model of intranasal challenge with Salmonella enterica serotype Enteritidis. Microbes Infect 6, 901–910, https://doi.org/10.1016/j.micinf.2004.05.007 (2004).

  17. 17.

    Apter, F. M., Lencer, W. I., Finkelstein, R. A., Mekalanos, J. J. & Neutra, M. R. Monoclonal immunoglobulin A antibodies directed against cholera toxin prevent the toxin-induced chloride secretory response and block toxin binding to intestinal epithelial cells in vitro. Infect Immun 61, 5271–5278 (1993).

  18. 18.

    Phalipon, A. et al. Monoclonal immunoglobulin A antibody directed against serotype-specific epitope of Shigella flexneri lipopolysaccharide protects against murine experimental shigellosis. J Exp Med 182, 769–778, https://doi.org/10.1084/jem.182.3.769 (1995).

  19. 19.

    van der Waaij, L. A., Limburg, P. C., Mesander, G. & van der Waaij, D. In vivo IgA coating of anaerobic bacteria in human faeces. Gut 38, 348–354, https://doi.org/10.1136/gut.38.3.348 (1996).

  20. 20.

    Tsuruta, T. et al. The amount of secreted IgA may not determine the secretory IgA coating ratio of gastrointestinal bacteria. FEMS Immunol Med Microbiol 56, 185–189, https://doi.org/10.1111/j.1574-695X.2009.00568.x (2009).

  21. 21.

    Kawamoto, S. et al. The inhibitory receptor PD-1 regulates IgA selection and bacterial composition in the gut. Science 336, 485–489, https://doi.org/10.1126/science.1217718 (2012).

  22. 22.

    van der Waaij, L. A. et al. Immunoglobulin coating of faecal bacteria in inflammatory bowel disease. Eur J Gastroenterol Hepatol 16, 669–674 (2004).

  23. 23.

    Robles Alonso, V. & Guarner, F. Linking the gut microbiota to human health. Br J Nutr 109(Suppl 2), S21–26, https://doi.org/10.1017/S0007114512005235 (2013).

  24. 24.

    Brandtzaeg, P. Secretory IgA: Designed for Anti-Microbial Defense. Front Immunol 4, 222, https://doi.org/10.3389/fimmu.2013.00222 (2013).

  25. 25.

    Brandtzaeg, P. Mucosal immunity: induction, dissemination, and effector functions. Scand J Immunol 70, 505–515, https://doi.org/10.1111/j.1365-3083.2009.02319.x (2009).

  26. 26.

    Brandtzaeg, P. Gate-keeper function of the intestinal epithelium. Benef Microbes 4, 67–82, https://doi.org/10.3920/BM2012.0024 (2013).

  27. 27.

    Yazdani, R., Azizi, G., Abolhassani, H. & Aghamohammadi, A. Selective IgA Deficiency: Epidemiology, Pathogenesis, Clinical Phenotype, Diagnosis, Prognosis and Management. Scand J Immunol 85, 3–12, https://doi.org/10.1111/sji.12499 (2017).

  28. 28.

    Loomes, L. M., Senior, B. W. & Kerr, M. A. A proteolytic enzyme secreted by Proteus mirabilis degrades immunoglobulins of the immunoglobulin A1 (IgA1), IgA2, and IgG isotypes. Infect Immun 58, 1979–1985 (1990).

  29. 29.

    Plaut, A. G., Gilbert, J. V., Artenstein, M. S. & Capra, J. D. Neisseria gonorrhoeae and neisseria meningitidis: extracellular enzyme cleaves human immunoglobulin A. Science 190, 1103–1105 (1975).

  30. 30.

    Moon, C. et al. Vertically transmitted faecal IgA levels determine extra-chromosomal phenotypic variation. Nature 521, 90–93, https://doi.org/10.1038/nature14139 (2015).

  31. 31.

    Julliard, W. et al. Amelioration of Clostridium difficile Infection in Mice by Dietary Supplementation With Indole-3-carbinol. Ann Surg 265, 1183–1191, https://doi.org/10.1097/SLA.0000000000001830 (2017).

  32. 32.

    Brawner, K. M. et al. Helicobacter pylori infection is associated with an altered gastric microbiota in children. Mucosal Immunol 10, 1169–1177, https://doi.org/10.1038/mi.2016.131 (2017).

  33. 33.

    Miyoshi, H. & Stappenbeck, T. S. In vitro expansion and genetic modification of gastrointestinal stem cells in spheroid culture. Nat Protoc 8, 2471–2482, https://doi.org/10.1038/nprot.2013.153 (2013).

  34. 34.

    Moon, C., VanDussen, K. L., Miyoshi, H. & Stappenbeck, T. S. Development of a primary mouse intestinal epithelial cell monolayer culture system to evaluate factors that modulate IgA transcytosis. Mucosal Immunol 7, 818–828, https://doi.org/10.1038/mi.2013.98 (2014).

  35. 35.

    Hubbard, T. D. et al. Dietary Broccoli Impacts Microbial Community Structure and Attenuates Chemically Induced Colitis in Mice in an Ah receptor dependent manner. J Funct Foods 37, 685–698, https://doi.org/10.1016/j.jff.2017.08.038 (2017).

  36. 36.

    Ozcam, M. et al. The gut symbionts Lactobacillus reuteri R2lc and 2010 encode a polyketide synthase cluster that activates the mammalian aryl-hydrocarbon receptor. Appl Environ Microbiol. https://doi.org/10.1128/AEM.01661-18 (2018).

  37. 37.

    Brandtzaeg, P. & Korsrud, F. R. Significance of different J chain profiles in human tissues: generation of IgA and IgM with binding site for secretory component is related to the J chain expressing capacity of the total local immunocyte population, including IgG and IgD producing cells, and depends on the clinical state of the tissue. Clin Exp Immunol 58, 709–718 (1984).

  38. 38.

    Brandtzaeg, P. & Prydz, H. Direct evidence for an integrated function of J chain and secretory component in epithelial transport of immunoglobulins. Nature 311, 71–73 (1984).

  39. 39.

    Mostov, K. E., Kraehenbuhl, J. P. & Blobel, G. Receptor-mediated transcellular transport of immunoglobulin: synthesis of secretory component as multiple and larger transmembrane forms. Proc Natl Acad Sci USA 77, 7257–7261 (1980).

  40. 40.

    Kaetzel, C. S. The polymeric immunoglobulin receptor: bridging innate and adaptive immune responses at mucosal surfaces. Immunol Rev 206, 83–99, https://doi.org/10.1111/j.0105-2896.2005.00278.x (2005).

  41. 41.

    Mostov, K. E., Verges, M. & Altschuler, Y. Membrane traffic in polarized epithelial cells. Curr Opin Cell Biol 12, 483–490 (2000).

  42. 42.

    Rojas, R. & Apodaca, G. Immunoglobulin transport across polarized epithelial cells. Nat Rev Mol Cell Biol 3, 944–955, https://doi.org/10.1038/nrm972 (2002).

  43. 43.

    Lindh, E. Increased risistance of immunoglobulin A dimers to proteolytic degradation after binding of secretory component. J Immunol 114, 284–286 (1975).

  44. 44.

    Craven, M. et al. Inflammation drives dysbiosis and bacterial invasion in murine models of ileal Crohn’s disease. PLoS One 7, e41594, https://doi.org/10.1371/journal.pone.0041594 (2012).

  45. 45.

    Schaubeck, M. et al. Dysbiotic gut microbiota causes transmissible Crohn’s disease-like ileitis independent of failure in antimicrobial defence. Gut 65, 225–237, https://doi.org/10.1136/gutjnl-2015-309333 (2016).

  46. 46.

    Gevers, D. et al. The treatment-naive microbiome in new-onset Crohn’s disease. Cell Host Microbe 15, 382–392, https://doi.org/10.1016/j.chom.2014.02.005 (2014).

  47. 47.

    Dey, N., Soergel, D. A., Repo, S. & Brenner, S. E. Association of gut microbiota with post-operative clinical course in Crohn’s disease. BMC Gastroenterol 13, 131, https://doi.org/10.1186/1471-230X-13-131 (2013).

  48. 48.

    Nguyen, T. L., Vieira-Silva, S., Liston, A. & Raes, J. How informative is the mouse for human gut microbiota research? Dis Model Mech 8, 1–16, https://doi.org/10.1242/dmm.017400 (2015).

  49. 49.

    Fleissner, C. K. et al. Absence of intestinal microbiota does not protect mice from diet-induced obesity. Br J Nutr 104, 919–929, https://doi.org/10.1017/S0007114510001303 (2010).

  50. 50.

    Turnbaugh, P. J., Backhed, F., Fulton, L. & Gordon, J. I. Diet-induced obesity is linked to marked but reversible alterations in the mouse distal gut microbiome. Cell Host Microbe 3, 213–223, https://doi.org/10.1016/j.chom.2008.02.015 (2008).

  51. 51.

    Truax, A. D. et al. The Inhibitory Innate Immune Sensor NLRP12 Maintains a Threshold against Obesity by Regulating Gut Microbiota Homeostasis. Cell Host Microbe 24, 364–378 e366, https://doi.org/10.1016/j.chom.2018.08.009 (2018).

  52. 52.

    Zhang, H. et al. Human gut microbiota in obesity and after gastric bypass. Proc Natl Acad Sci USA 106, 2365–2370, https://doi.org/10.1073/pnas.0812600106 (2009).

  53. 53.

    Hu, Y., Peng, J., Li, F., Wong, F. S. & Wen, L. Evaluation of different mucosal microbiota leads to gut microbiota-based prediction of type 1 diabetes in NOD mice. Sci Rep 8, 15451, https://doi.org/10.1038/s41598-018-33571-z (2018).

  54. 54.

    Gupta, S., Basu, S., Bal, V., Rath, S. & George, A. Gut IgA abundance in adult life is a major determinant of resistance to dextran sodium sulfate-colitis and can compensate for the effects of inadequate maternal IgA received by neonates. Immunology, https://doi.org/10.1111/imm.13091 (2019).

  55. 55.

    Agus, A., Planchais, J. & Sokol, H. Gut Microbiota Regulation of Tryptophan Metabolism in Health and Disease. Cell Host Microbe 23, 716–724, https://doi.org/10.1016/j.chom.2018.05.003 (2018).

  56. 56.

    Safe, S., Papineni, S. & Chintharlapalli, S. Cancer chemotherapy with indole-3-carbinol, bis(3′-indolyl)methane and synthetic analogs. Cancer Lett 269, 326–338, https://doi.org/10.1016/j.canlet.2008.04.021 (2008).

  57. 57.

    Auborn, K. J. et al. Lifespan is prolonged in autoimmune-prone (NZB/NZW) F1 mice fed a diet supplemented with indole-3-carbinol. J Nutr 133, 3610–3613, https://doi.org/10.1093/jn/133.11.3610 (2003).

  58. 58.

    Kim, Y. H. et al. 3,3′-diindolylmethane attenuates colonic inflammation and tumorigenesis in mice. Inflamm Bowel Dis 15, 1164–1173, https://doi.org/10.1002/ibd.20917 (2009).

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Acknowledgements

We thank Dr. Greg Kennedy and Dr. Christopher Graham for kindly providing the HCT116 reporter cell line and providing technical consultation for the luciferase assay protocol. We also thank Dr. Marie Nearing and Dr. Katie Alexander of the UAB Organogenesis Unit for sharing technical expertise related to spheroid culturing as well as the laboratory of Dr. Francis Lund for the use of its luminometer. The Targeted Metabolomics and Proteomics Laboratory at UAB provided assistance obtaining the metabolomics data presented in this work. Purchase of the SCIEX 5600 TripleTof Mass Spectrometer in the Targeted Metabolomics and Proteomics Laboratory came from funds provided by the NIH S10 RR027822-01 grant. Funds for the operation of the Targeted Metabolomics and Proteomics Laboratory come in part from the UAB O’Brien Acute Kidney Injury Center (P30 DK079337). This work was funded by grants to C.A.M. from the Kaul Pediatric Research Institute and the Surgical Society of the Alimentary Tract. L.E.S. is supported by the Broad Medical Foundation and the Crohn’s and Colitis Foundation of America. This publication was also made possible by the UAB Center for Clinical and Translational Science Grant Number UL1TR001417 from the National Center for Advancing Translational Sciences (NCATS) of the National Institutes of Health (NIH).

Author information

C.A.M. conceived and supervised the study. K.M.B. and V.A.Y. performed the experiments. L.W.D. assisted with bacterial anaerobic culturing. K.M.B. and W.V.D.P. analyzed the data. L.E.S., C.D.M., and C.O.E. offered helpful ideas for experimental design and troubleshooting. K.M.B. and C.A.M. wrote the manuscript. All authors reviewed the manuscript.

Correspondence to Kyle M. Brawner.

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Brawner, K.M., Yeramilli, V.A., Duck, L.W. et al. Depletion of dietary aryl hydrocarbon receptor ligands alters microbiota composition and function. Sci Rep 9, 14724 (2019) doi:10.1038/s41598-019-51194-w

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