- Open Access
Type 2 immunity-dependent reduction of segmented filamentous bacteria in mice infected with the helminthic parasite Nippostrongylus brasiliensis
© Fricke et al. 2015
- Received: 23 June 2015
- Accepted: 17 August 2015
- Published: 17 September 2015
The Erratum to this article has been published in Microbiome 2015 3:77
Dynamic interactions between the host and gastrointestinal microbiota play an important role for local and systemic immune homeostasis. Helminthic parasites modulate the host immune response, resulting in protection against autoimmune disease but also increased susceptibility to pathogen infection. The underlying mechanisms remain largely unknown.
We showed that the type 2 immune response to enteric Nippostrongylus brasiliensis infection in mice was associated with altered intestinal mucin and AMP expression and shifts in microbiota composition. Most strikingly, infection reduced concentrations of intestinal segmented filamentous bacteria (SFB), known inducers of T helper 17 cells, and IL-17-associated gene expression. Infected mice deficient in IL-13 or STAT6 did not reduce SFB or IL-17, and exogenous IL-25 replicated the effects of parasite infection in wild type mice.
Our data show that parasite infection acts through host type 2 immunity to reduce intestinal SFB and expression of IL-17, providing an example of a microbiota-dependent immune modulation by parasites.
- Helminth parasite
- Nippostrongylus brasiliensis
- Type 2 immunity
- Antimicrobial peptides
- Segmented filamentous bacteria
Homeostasis of the mammalian gastrointestinal (GI) tract depends on a complex network of interactions between the host and microbiota, including parasitic nematodes, bacteria, viruses, and others . To describe the potential of individual microbiota members to exert both beneficial and detrimental effects on the host, the term “pathobiont” has been suggested for symbiotic organisms that induce pathology under certain conditions . For example, segmented filamentous bacteria (SFB), Gram-positive members of the Clostridiaceae family that colonize various vertebrate species including humans [3, 4], promote specific T helper (Th)17 differentiation through MHCII-dependent antigen presentation by intestinal dendritic cells [5, 6]. Mono-colonization with SFB can restore immune deficits of germ-free mice, including induction of germinal center activation in Peyer’s patches, production of immunoglobulin A, and T cell expansion . SFB induce genes associated with inflammation and antimicrobial defenses and increase resistance to the intestinal bacterial pathogen Citrobacter rodentium . However, SFB also promote extra-intestinal Th17 responses during autoimmune disease, including autoimmune arthritis in the K/BxN mouse model  and experimental autoimmune encephalomyelitis (EAE), a murine model of multiple sclerosis . In addition, non-alcoholic fatty liver disease (NAFLD), a common inflammation-driven sequela of obesity, can be exacerbated or prevented in mice by colonization or antibiotic depletion of SFB, respectively .
There has been growing interest in understanding the multilayered crosstalk and interactions between nematodes, commensal bacteria, and the host immune system given differences in disease expression in human populations where enteric helminth parasite infection is controlled compared to where it persists . Nematode infection induces polarized type 2 immunity characterized by increased expression of cytokines such as IL-4, IL-5, IL-13, and IL-25 . Epithelial-derived IL-25 is believed to be an initiating factor for the immune cascade, which stimulates type 2 innate lymphoid cells (ILC2) to release IL-5 and IL-13. Host defense against nematode infection relies on Th2 cytokines IL-4 and IL-13 activating STAT6 signaling pathways, which then leads to up-regulation of various downstream effector molecules as well as stereotypic alterations in gut function. Parasite nematodes also have the capacity to suppress Th1 or Th17 immune responses that influence susceptibility to microbial pathogens as well as the process of autoimmunity. For example, concurrent infection with the parasitic nematode Heligmosomoides polygyrus bakeri increased the susceptibility of mice to C. rodentium . On the other hand, helminth infection can prevent type 1 diabetes, EAE, Graves’ disease, collagen-induced arthritis, and inflammatory bowel disease (IBD) , protect against allergies [15, 16], and improve symptoms in IBD [17, 18], all of which are Th1/Th17-associated inflammatory or autoimmune diseases. So far, the cellular and molecular mechanisms underlying the potent immune modulating activities of nematodes remain elusive.
We sought to investigate the effects of infection with the parasitic model nematode Nippostrongylus brasiliensis on the composition of the gut microbiota focusing on segmented filamentous bacteria (SFB), a specific Th17-eliciting commensal bacterium, with the goal to gain mechanistic insight into the immune modulating role of parasitic nematodes. Our data showed, for the first time, that the host type 2 response to parasitic nematode infection can inhibit intestinal SFB and decrease the expression of IL-17-associated genes, possible via modulation of antimicrobial peptide and mucin expression.
Nippostrongylus brasiliensis infection induces type 2 immunity and changes the expression of antimicrobial peptides and mucins in the small intestine
To determine whether N. brasiliensis infection altered the gene expression of antimicrobial peptides (AMP) and mucins in the ileum, we analyzed samples from mice collected at day 11 post-inoculation. The infection up-regulated the expression of resistin-like molecule beta (Retnlb), angiogenin 4 (Ang4), and mucin 2 (Muc2) but down-regulated regenerating islet-derived protein 3 gamma (Reg3γ) and lysozymes 1 (Lyz1) and 2 (Lyz2) (Fig. 1c). Expression of mucin 5 AC (Muc5AC), a pivotal player for worm expulsion , or defensin alpha 1 (Defa1) was not affected by the infection at this time (Fig. 1c).
Infection with N. brasiliensis reduces Firmicutes but increases Bacteroidetes and Actinobacteria in the ileum
Infection with N. brasiliensis also correlated with significant changes in the abundance of the three dominant bacterial phyla Firmicutes (98.7 ± 0.6 % in uninfected versus 94.7 ± 1.6 % in infected mice) Bacteroidetes (0.9 ± 0.4 % in uninfected versus 3.7 ± 1.1 % in infected mice) and Actinobacteria (0.1 ± 0.03 % in uninfected versus 1 ± 0.4 % in infected mice) (Fig. 2d). Among the Firmicutes, N. brasiliensis infection significantly increased the abundance of Lactobacillaceae but decreased the abundance of Peptostreptococcaceae, Clostridiaceae, and Turicibacteraceae (Fig. 2e). Members of the taxonomic families S24-7 and Coriobacteriaceae of the Bacteroidetes and Actinobacteria, respectively, were significantly increased in N. brasiliensis-infected compared to uninfected mice.
Abundance of SFB and expression of IL-17-associated genes are reduced in N. brasiliensis-infected mice
We sought to examine the expression of host IL-17-associated genes in ileal tissue of N. brasiliensis-infected mice because helminthic infection has been shown to inhibit pro-inflammatory Th1/Th17 responses [22, 12]. Transcript levels of all tested IL-17-associated genes were significantly lower in ileal tissues from N. brasiliensis-infected compared to uninfected mice, including IL-17A, IL-17C, IL-17F, IL-17RA, IL-22, as well as Th17-inducing serum amyloid A proteins SAA1 and SAA2 (Fig. 3f).
Infection of SFB-negative mice with N. brasiliensis does not affect ileal IL-17 expression
N. brasiliensis-induced modulation of AMP, SFB, and IL-17 depends on host IL-13/STAT6 axis
Exogenous IL-25 modulates AMP, SFB, and IL-17 gene expression similar to infection with N. brasiliensis
Subsequently, exogenous IL-25 was injected to IL-13−/− mice. In contrast to what was observed in WT mice, administration of IL-25 to IL-13−/− mice did not modulate ileal expression of Ang4, Reg3γ, or Lyz1 but down-regulate Retnlb (Fig. 6d). Consistent with these results, IL-25 had no significant effect on ileal SFB in IL-13−/− mice (Fig. 6e). Although exogenous IL-25 down-regulated the expression of IL-17 F and IL-22 in IL-13−/− mice, albeit to a lesser degree than in WT mice, the inhibitory effects of IL-25 in WT mice on the key IL-17-associated genes IL-17A and IL-17C disappeared in IL-13−/− mice. An up-regulation of IL-17A, IL-17C, and SAA1 was detected in IL-25-treated IL-13−/− mice (Fig. 6f).
The effects of nematode infection on the intestinal microbiota have been studied with differing results in humans. While various types of helminth infection were associated with altered microbiota composition in a Malaysian indigenous community , as well as in children from Ecuador colonized with Trichuris trichiura and Ascaris lumbricoides but not T. trichiura alone , no measurable effect on the microbiota structure was seen in participants of a clinical study infected with Necator americanus . In summary, additional studies using larger, more standardized patient cohorts and localized tissue sampling may be required [28, 29] to identify potential effects of parasite infection on the human intestinal microbiota.
Host-derived mucins and AMP control the composition and spatial organization of the intestinal microbiota and are induced in response to parasite and other enteric infections . Resistin-like molecule β (Retnlb), for example, provides protection against N. brasiliensis and H. polygyrus in mice, independently of T or B cells or M2 macrophages, by interfering with the parasite’s ability to feed on host tissue during infection . Mucin glycoproteins secreted by goblet cells concentrate AMP produced by Paneth cells and protect the intestinal lining from direct contact with luminal microorganism. Proliferation of intestinal goblet cells is a prominent feature of the type 2 immune response to nematode infection [32, 33] and both Muc2 and Muc5ac are important for worm expulsion [20, 34]. At the same time, mucus-derived glycans are an important energy source for intestinal bacteria . We found the expression of Muc2 and several AMP with broad antimicrobial activity to be altered in response to N. brasiliensis infection, including Ang4 (effective against Gram-positive/-negative bacteria), Reg3γ (effective against Gram-positive bacteria), and Lyz1 and Lyz2 (mostly effective against Gram-positive bacteria) . Together, our results suggest that parasite-induced changes to intestinal mucus architecture and AMP expression profiles could be responsible for the altered intestinal microbiota observed in parasite-infected mice.
Notably, our observed increase in Lactobacillaceae in the ileum of N. brasiliensis-infected mice was consistent with a similar increase found in ileal but not cecal samples of H. polygyrus-infected mice . To our knowledge, however, our study is the first to report a reduction in SFB in response to parasite infection, a bacterial species that has received widespread attention due to its unique Th17-inducing and immune modulating capabilities.
Parasite expulsion is associated with smooth muscle hyper-contractility, epithelial cell hypo-secretion, and increased mucosal permeability, mediated primarily via IL-4/IL-13 and receptor-mediated activation of STAT6 signaling pathways [35, 36]. As IL-13−/− mice fail to reduce SFB and IL-17A expression in response to N. brasiliensis infection, IL-4 appears unable to compensate for IL-13 with regard to its role for SFB and IL-17-dependent immune modulation. Because SFB colonize the ileal intestinal wall , reduced concentrations of SFB in N. brasiliensis-infected mice could result from increased physical shedding of the intestinal mucus or from selectively increased AMP expression . Germ-free mice mono-colonized with SFB have been shown to induce Reg3γ , suggesting that the reduced Reg3γ expression in mice infected with N. brasiliensis was associated with lower SFB colonization or with distinct host cytokine regulatory pathways activated by parasite infection. Reduced levels of Reg3γ could affect the Gram-positive intestinal microbiota and lead to the increase in Lactobacillaceae observed in N. brasiliensis-infected mice. Mucosal IgA levels could also play a role for maintaining SFB homeostasis, as mice deficient for IgA, as well as mice that lack the TLR adaptor MyD88 in Treg cells, which results in impaired intestinal IgA responses, show an expansion of intestinal SFB [40, 41]. Our findings suggest complex interactions between parasite, host response, and microbiota that require further study.
Helminth infection impairs the human immune response to oral cholerae , tuberculosis vaccine BCG  and exacerbates Salmonella enterica Typhimurium pathogenicity in mice . Moreover, human Th17 responses to latent tuberculosis infection are reduced in individuals colonized with helminths [45, 46], with clinical consequences for large parts of the developing world where Mycobacterium tuberculosis and helminth infections are co-endemic . Suppression of Th1 and Th17 responses as well as attenuation of EAE, a murine model of the human autoimmune disease multiple sclerosis, was maintained in IL-10 knock-out mice infected with the liver fluke Fasciola hepatica . In H. polygyrus-infected mice, IL-17 suppression was not affected by blocking of IL-10 alone but by blocking of both IL-10 and the Th2 cytokine IL-4 . Our findings that parasite-induced IL-17 suppression is dependent on the IL-13/STAT6 axis and inducible solely by administration of IL-25 which also reduced SFB levels support and extend the link between Th2 and Th17 responses during parasite infection and help explain increased comorbidity to bacterial infections in parasite-infested individuals.
Parasite infection and colonization with SFB have been associated with beneficial and detrimental effects as results of opposing immune modulating roles, i.e., increased susceptibility to microbial infection and protection from inflammatory disorders in the case of parasite infection and increased resistance to some microbial infection and susceptibility to inflammatory disease in case of SFB. Our finding that parasite infection reduced the abundance of SFB and IL-17 activation could help explain epidemiological reports of negative correlations between parasite infection and autoimmune disease  as well as the success seen in the treatment of some inflammatory and autoimmune diseases with helminth therapy .
In light of the pro-inflammatory role of IL-17 for autoimmune disease, IL-17-inducing SFB could represent a valuable therapeutic target. However, only a few factors have been described that control SFB abundance and the mechanisms that are responsible for SFB regulation are largely unknown: Immune system deficiencies including loss of function of the MyD88 adaptor protein  used by most Toll-like receptors , lymphotoxin (TNFβ)  required for normal mucosal immunity , and the aryl hydrocarbon receptor  involved in the activation of group 3 ILCs  have been associated with increased intestinal SFB concentrations in mice. Shi et al. showed that IL-23 dynamically regulated SFB, as perturbation of the IL-23 pathway led to defective intestinal barrier function, systematic dissemination of microbial products, and altered antimicrobial activities .
C57BL/6 WT mice were purchased from NCI-Frederick Animal Production Program (Frederick, MD) and bred in the USDA/Beltsville animal facility. These mice were confirmed to be SFB positive by both 16S pyrosequencing and qPCR. SFB-negative WT mice in C57BL/6 background were purchased from Jackson Laboratory (Bar Harbor, ME). Jackson mice were housed in autoclaved cages in our closed container facility that have a sealed top and force-filtered air, feed autoclaved chow and water, handled in a biological safety hood with HEPA-filtered air, and used 1 week after arriving. Mice deficient in STAT6 (STAT6−/−) on C57BL/6 background from Jackson laboratory and mice deficient in IL-13 (IL-13−/−) from the NIAID Taconic contract were bred in the USDA/Beltsville animal facility. Both STAT6−/− and IL-13−/− mice were confirmed to be SFB positive before use. In general, mice were co-housed for 1 week before initiating treatment/infection to eliminate cage effects. Unless otherwise indicated, 8–12-week-old female mice were used throughout the study with 5–10 per group based on our previous studies using N. brasiliensis infection . Mice were randomly assigned to different treatment groups. Investigators were aware of the group allocation throughout the experiment. These studies were conducted with institutional approval from both the University of Maryland, Baltimore and the USDA Beltsville Area Institutional Animal Care and Use Committees, in accordance with principles set forth in the Guide for Care and Use of Laboratory Animals, Institute of Laboratory Animal Resources, National Research Council, Health and Human Services Publication (National Institutes of Health 85–23, revised 1996).
Infection of mice with N. brasiliensis
Infective, third-stage larvae of N. brasiliensis (specimens on file at the U.S. National Parasite Collection, U.S. National Helminthological Collection, Collection 81930, Beltsville, MD) were propagated and stored at room temperature in fecal/charcoal/peat moss culture plates until used. Groups of mice were inoculated subcutaneously with 500 third-stage larvae (L3) and euthanized at day 11 post-N. brasiliensis infection when immunocompetent mice cleared worms, as described previously . Appropriate age- and sex-matched WT or mice treated with vehicle were performed for each infection.
Administration of IL-25
For administration of IL-25, mice were injected i.p. with 1 μg of mouse recombinant IL-25, containing BSA as a carrier (Biolegend, CA) in 100-μl saline daily for 3 days or, as a control, injected with 35-μg BSA, which is equal to the amount of BSA included in the IL-25 preparation. The amount of cytokine administered was based on the effective dose of IL-25 that induced a prominent Th2 immune response from a previous study51.
Nucleic acid extraction and qPCRs
Intestinal strips containing the entire luminal contents were placed in RNAlater (Sigma-Aldrich, St. Louis, MO) and stored at −80 °C until processing. Prior to processing, samples were vortexed vigorously for 15 s and used for total DNA (supernatant) or RNA (tissue) isolation. Total RNA was extracted from mid-jejunum or ileum whole tissue and used for cDNA generation and real-time quantitative PCR (qPCR) as described previously . RNA samples (2 μg) were reverse transcribed to cDNA using the First Strand cDNA Synthase Kit (MBI Fermentas, Hanover, MD) with random hexamer primer. Real-time qPCR (qPCR) was performed on a CFX96 detection system (Bio-Rad, Hercules, CA). PCR was performed in a 25-μl volume using SYBR Green Supermix (Bio-Rad). Amplification conditions were: 95 °C for 3 min, 50 cycles of 95 °C for 15 s, 60 °C for 15 s, and 72 °C for 20 s. The fold changes in mRNA expressions for targeted genes were relative to the respective vehicle groups of mice after normalization to 18S rRNA. Primers were synthesized by Sigma-Aldrich. Results are presented as mean values and standard error of the mean (mean ± s.e.m.). Metagenomic DNA was isolated from mouse intestine or fecal pellets using the protocol for human fecal DNA isolation described in Song et al. , which includes both enzymatic digestions (lysozyme, mutanolysin, lysostaphin, proteinase K, and RNase) and mechanical disruption by bead beating. Segmented filamentous bacteria were quantified by qPCR using primer pairs specific for the SFB 16S rRNA gene or, for normalization, 16S rRNA genes from all bacteria as described in Barman et al. . Fifty nanograms of DNA template was amplified using the SYBR Green PCR Master Mix (Life Technologies, Carlsbad, CA) in a 10-μl reaction mix following the default amplification protocol of the ABI 7900HT Real-Time PCR system (Life Technologies). For SFB, relative quantity was calculated by the ΔCt method and normalized by counts for total bacteria. Typical Ct values for SFB were ~30 cycles and for total bacteria ~15 cycles. Concentrations for samples that were negative after 40 cycles were designated “not detectable” (n.d.).
16S rRNA gene amplification, sequencing, and microbiota analysis
Barcoded 16S rRNA gene PCR amplicons for sequencing were generated a described previously . Hypervariable regions V3 and V4 of the bacterial 16S rRNA gene were amplified with the universal primers 338F and 806R (amplicon length: ~470 bp). Reads spanning hypervariable region V3 were sequenced with primer 338 on the Illumina MiSeq platform. Quality trimming was performed as described before , using the following criteria: (1) reads were truncated upstream of >2 consecutive low-quality bases; (2) no reads with ambiguous base calls were used; and (3) reads with <150 bp after trimming were discarded. Quality trimming and demultiplexing were performed with QIIME (version 1.6.0) , resulting in between 3058 and 17,643 reads per sample. Sequences were clustered as operational taxonomic units (OTUs) based on a 97 % cutoff with USEARCH, de-novo chimera detection and removal were conducted with UCHIME v5.1 as implemented in QIIME. Taxonomic ranks were assigned to each sequence with the Ribosomal Database Project (RDP) Naïve Bayesian Classifier v.2.2, using a pre-built Greengenes database of 16S rRNA sequences [May, 2013] and a confidence value cutoff of 0.9, also as implemented in QIIME. Differentially abundant OTUs were determined with Metastats . Raw sequences of all non-chimeric reads that passed the quality trimming were deposited in the NCBI Short Read Archive under accession numbers SRA176950 and SRP045195 (Bioproject ID: PRJNA255974).
The Shapiro-Wilk test was used to evaluate the normality of the obtained data. Outliers were identified using the ROUT method and excluded from the analysis. If necessary, variance between compared groups was corrected with the Geisser-Greenhouse method. One-way ANOVA followed by Newman-Keuls test was performed for comparisons of more than two groups. When normal distribution was satisfied, Student’s t-test was used for comparing differences between groups. Otherwise, the non-parametric Mann–Whitney test was used. All analyses and plots were conducted using Prism (version 6 for Mac, GraphPad Software, San Diego, CA, USA). Results are presented as mean ± s.e.m. Statistical significance was declared if the two-sided P value was <0.05.
This work was supported by the Carl-Zeiss-Stiftung/German Scholars Organization e.V. (WFF: Wissenschaftler-Rückkehrprogramm GSO/CZS), the U.S. National Institutes of Health (AZ: R01-DK083418, T.S-D: R01-AI/DK49316), the U.S. Department of Agriculture (AS, JFU: CRIS #1235-51000-055), and the Chinese State Scholarship Fund (AJW: #201208360042).
The funding organizations had no role in study design, in the collection, analysis, and interpretation of data; in the writing of the manuscript; and in the decision to submit the manuscript for publication.
The opinions and assertions in this article are those of the authors and do not necessarily represent those of the U. S. Department of Agriculture (USDA). Mention of trade names or commercial products in this publication is solely for the purpose of providing specific information and does not imply recommendation or endorsement by the USDA. The USDA is an equal opportunity provider and employer.
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- Hooper LV, Littman DR, Macpherson AJ. Interactions between the microbiota and the immune system. Science. 2012;336(6086):1268–73. doi:10.1126/science.1223490.View ArticlePubMed CentralPubMedGoogle Scholar
- Chow J, Tang H, Mazmanian SK. Pathobionts of the gastrointestinal microbiota and inflammatory disease. Curr Opin Immunol. 2011;23(4):473–80. doi:10.1016/j.coi.2011.07.010.View ArticlePubMed CentralPubMedGoogle Scholar
- Davis CP, Savage DC. Habitat, succession, attachment, and morphology of segmented, filamentous microbes indigenous to the murine gastrointestinal tract. Infect Immun. 1974;10(4):948–56.PubMed CentralPubMedGoogle Scholar
- Yin Y, Wang Y, Zhu L, Liu W, Liao N, Jiang M, et al. Comparative analysis of the distribution of segmented filamentous bacteria in humans, mice and chickens. ISME J. 2013;7(3):615–21. doi:10.1038/ismej.2012.128.View ArticlePubMed CentralPubMedGoogle Scholar
- Ivanov II, Atarashi K, Manel N, Brodie EL, Shima T, Karaoz U, et al. Induction of intestinal Th17 cells by segmented filamentous bacteria. Cell. 2009;139(3):485–98. doi:10.1016/j.cell.2009.09.033.View ArticlePubMed CentralPubMedGoogle Scholar
- Goto Y, Panea C, Nakato G, Cebula A, Lee C, Diez MG, et al. Segmented filamentous bacteria antigens presented by intestinal dendritic cells drive mucosal Th17 cell differentiation. Immunity. 2014;40(4):594–607. doi:10.1016/j.immuni.2014.03.005.View ArticlePubMed CentralPubMedGoogle Scholar
- Lee YK, Mazmanian SK. Microbial learning lessons: SFB educate the immune system. Immunity. 2014;40(4):457–9. doi:10.1016/j.immuni.2014.04.002.View ArticlePubMedGoogle Scholar
- Ivanov II WHJ, Darce J, Hattori K, Shima T, Umesaki Y, et al. Gut-residing segmented filamentous bacteria drive autoimmune arthritis via T helper 17 cells. Immunity. 2010;32(6):815–27. doi:10.1016/j.immuni.2010.06.001.View ArticlePubMed CentralPubMedGoogle Scholar
- Lee YK, Menezes JS, Umesaki Y, Mazmanian SK. Proinflammatory T-cell responses to gut microbiota promote experimental autoimmune encephalomyelitis. Proc Natl Acad Sci U S A. 2011;108 Suppl 1:4615–22. doi:10.1073/pnas.1000082107.View ArticlePubMed CentralPubMedGoogle Scholar
- Harley IT, Stankiewicz TE, Giles DA, Softic S, Flick LM, Cappelletti M, et al. IL-17 signaling accelerates the progression of nonalcoholic fatty liver disease in mice. Hepatology. 2014;59(5):1830–9. doi:10.1002/hep.26746.View ArticlePubMed CentralPubMedGoogle Scholar
- Salgame P, Yap GS, Gause WC. Effect of helminth-induced immunity on infections with microbial pathogens. Nat Immunol. 2013;14(11):1118–26. doi:10.1038/ni.2736.View ArticlePubMedGoogle Scholar
- McSorley HJ, Maizels RM. Helminth infections and host immune regulation. Clin Microbiol Rev. 2012;25(4):585–608. doi:10.1128/CMR.05040-11.View ArticlePubMed CentralPubMedGoogle Scholar
- Chen CC, Louie S, McCormick B, Walker WA, Shi HN. Concurrent infection with an intestinal helminth parasite impairs host resistance to enteric Citrobacter rodentium and enhances Citrobacter-induced colitis in mice. Infect Immun. 2005;73(9):5468–81. doi:10.1128/IAI.73.9.5468-5481.2005.View ArticlePubMed CentralPubMedGoogle Scholar
- Zaccone P, Cooke A. Vaccine against autoimmune disease: can helminths or their products provide a therapy? Curr Opin Immunol. 2013;25(3):418–23. doi:10.1016/j.coi.2013.02.006.View ArticlePubMedGoogle Scholar
- Endara P, Vaca M, Chico ME, Erazo S, Oviedo G, Quinzo I, et al. Long-term periodic anthelmintic treatments are associated with increased allergen skin reactivity. Clin Exp Allergy. 2010;40(11):1669–77. doi:10.1111/j.1365-2222.2010.03559.x.View ArticlePubMed CentralPubMedGoogle Scholar
- Rodrigues LC, Newcombe PJ, Cunha SS, Alcantara-Neves NM, Genser B, Cruz AA, et al. Early infection with Trichuris trichiura and allergen skin test reactivity in later childhood. Clin Exp Allergy. 2008;38(11):1769–77. doi:10.1111/j.1365-2222.2008.03027.x.PubMedGoogle Scholar
- Summers RW, Elliott DE, Urban Jr JF, Thompson R, Weinstock JV. Trichuris suis therapy in Crohn’s disease. Gut. 2005;54(1):87–90. doi:10.1136/gut.2004.041749.View ArticlePubMed CentralPubMedGoogle Scholar
- Summers RW, Elliott DE, Urban Jr JF, Thompson RA, Weinstock JV. Trichuris suis therapy for active ulcerative colitis: a randomized controlled trial. Gastroenterology. 2005;128(4):825–32.View ArticlePubMedGoogle Scholar
- Finkelman FD, Shea-Donohue T, Goldhill J, Sullivan CA, Morris SC, Madden KB, et al. Cytokine regulation of host defense against parasitic gastrointestinal nematodes: lessons from studies with rodent models. Annu Rev Immunol. 1997;15:505–33. doi:10.1146/annurev.immunol.15.1.505.View ArticlePubMedGoogle Scholar
- Hasnain SZ, Evans CM, Roy M, Gallagher AL, Kindrachuk KN, Barron L, et al. Muc5ac: a critical component mediating the rejection of enteric nematodes. J Exp Med. 2011;208(5):893–900. doi:10.1084/jem.20102057.View ArticlePubMed CentralPubMedGoogle Scholar
- Walk ST, Blum AM, Ewing SA, Weinstock JV, Young VB. Alteration of the murine gut microbiota during infection with the parasitic helminth Heligmosomoides polygyrus. Inflamm Bowel Dis. 2010;16(11):1841–9. doi:10.1002/ibd.21299.View ArticlePubMed CentralPubMedGoogle Scholar
- Finlay CM, Walsh KP, Mills KH. Induction of regulatory cells by helminth parasites: exploitation for the treatment of inflammatory diseases. Immunol Rev. 2014;259(1):206–30. doi:10.1111/imr.12164.View ArticlePubMedGoogle Scholar
- Kolls JK, McCray Jr PB, Chan YR. Cytokine-mediated regulation of antimicrobial proteins. Nat Rev Immunol. 2008;8(11):829–35. doi:10.1038/nri2433.View ArticlePubMed CentralPubMedGoogle Scholar
- Owyang AM, Zaph C, Wilson EH, Guild KJ, McClanahan T, Miller HR, et al. Interleukin 25 regulates type 2 cytokine-dependent immunity and limits chronic inflammation in the gastrointestinal tract. J Exp Med. 2006;203(4):843–9. doi:10.1084/jem.20051496.View ArticlePubMed CentralPubMedGoogle Scholar
- Lee SC, Tang MS, Lim YA, Choy SH, Kurtz ZD, Cox LM, et al. Helminth colonization is associated with increased diversity of the gut microbiota. PLoS Negl Trop Dis. 2014;8(5), e2880. doi:10.1371/journal.pntd.0002880.View ArticlePubMed CentralPubMedGoogle Scholar
- Cooper P, Walker AW, Reyes J, Chico M, Salter SJ, Vaca M, et al. Patent human infections with the whipworm, Trichuris trichiura, are not associated with alterations in the faecal microbiota. PLoS One. 2013;8(10), e76573. doi:10.1371/journal.pone.0076573.View ArticlePubMed CentralPubMedGoogle Scholar
- Cantacessi C, Giacomin P, Croese J, Zakrzewski M, Sotillo J, McCann L et al. Impact of experimental hookworm infection on the human gut microbiota. J Infect Dis. 2014. doi:10.1093/infdis/jiu256.
- Li RW, Wu S, Li W, Navarro K, Couch RD, Hill D, et al. Alterations in the porcine colon microbiota induced by the gastrointestinal nematode Trichuris suis. Infect Immun. 2012;80(6):2150–7. doi:10.1128/IAI.00141-12.View ArticlePubMed CentralPubMedGoogle Scholar
- Wu S, Li RW, Li W, Beshah E, Dawson HD, Urban Jr JF. Worm burden-dependent disruption of the porcine colon microbiota by Trichuris suis infection. PLoS One. 2012;7(4):e35470. doi:10.1371/journal.pone.0035470.View ArticlePubMed CentralPubMedGoogle Scholar
- Gallo RL, Hooper LV. Epithelial antimicrobial defence of the skin and intestine. Nat Rev Immunol. 2012;12(7):503–16. doi:10.1038/nri3228.View ArticlePubMed CentralPubMedGoogle Scholar
- Herbert DR, Yang JQ, Hogan SP, Groschwitz K, Khodoun M, Munitz A, et al. Intestinal epithelial cell secretion of RELM-beta protects against gastrointestinal worm infection. J Exp Med. 2009;206(13):2947–57. doi:10.1084/jem.20091268.View ArticlePubMed CentralPubMedGoogle Scholar
- Allen JE, Maizels RM. Diversity and dialogue in immunity to helminths. Nat Rev Immunol. 2011;11(6):375–88. doi:10.1038/nri2992.View ArticlePubMedGoogle Scholar
- Artis D, Grencis RK. The intestinal epithelium: sensors to effectors in nematode infection. Mucosal Immunol. 2008;1(4):252–64. doi:10.1038/mi.2008.21.View ArticlePubMedGoogle Scholar
- Johansson ME, Larsson JM, Hansson GC. The two mucus layers of colon are organized by the MUC2 mucin, whereas the outer layer is a legislator of host-microbial interactions. Proc Natl Acad Sci U S A. 2011;108 Suppl 1:4659–65. doi:10.1073/pnas.1006451107.View ArticlePubMed CentralPubMedGoogle Scholar
- Akiho H, Blennerhassett P, Deng Y, Collins SM. Role of IL-4, IL-13, and STAT6 in inflammation-induced hypercontractility of murine smooth muscle cells. Am J Physiol Gastrointest Liver Physiol. 2002;282(2):G226–32.PubMedGoogle Scholar
- Zhao A, McDermott J, Urban Jr JF, Gause W, Madden KB, Yeung KA, et al. Dependence of IL-4, IL-13, and nematode-induced alterations in murine small intestinal smooth muscle contractility on Stat6 and enteric nerves. J Immunol. 2003;171(2):948–54.View ArticlePubMedGoogle Scholar
- Koopman JP, Stadhouders AM, Kennis HM, De Boer H. The attachment of filamentous segmented micro-organisms to the distal ileum wall of the mouse: a scanning and transmission electron microscopy study. Lab Anim. 1987;21(1):48–52.View ArticlePubMedGoogle Scholar
- Vaishnava S, Yamamoto M, Severson KM, Ruhn KA, Yu X, Koren O, et al. The antibacterial lectin RegIIIgamma promotes the spatial segregation of microbiota and host in the intestine. Science. 2011;334(6053):255–8. doi:10.1126/science.1209791.View ArticlePubMed CentralPubMedGoogle Scholar
- Keilbaugh SA, Shin ME, Banchereau RF, McVay LD, Boyko N, Artis D, et al. Activation of RegIIIbeta/gamma and interferon gamma expression in the intestinal tract of SCID mice: an innate response to bacterial colonisation of the gut. Gut. 2005;54(5):623–9. doi:10.1136/gut.2004.056028.View ArticlePubMed CentralPubMedGoogle Scholar
- Suzuki K, Meek B, Doi Y, Muramatsu M, Chiba T, Honjo T, et al. Aberrant expansion of segmented filamentous bacteria in IgA-deficient gut. Proc Natl Acad Sci U S A. 2004;101(7):1981–6. doi:10.1073/pnas.0307317101.View ArticlePubMed CentralPubMedGoogle Scholar
- Wang S, Charbonnier LM, Noval Rivas M, Georgiev P, Li N, Gerber G et al. MyD88 adaptor-dependent microbial sensing by regulatory T cells promotes mucosal tolerance and enforces commensalism. Immunity. 2015. doi:10.1016/j.immuni.2015.06.014.
- Cooper PJ, Chico M, Sandoval C, Espinel I, Guevara A, Levine MM, et al. Human infection with Ascaris lumbricoides is associated with suppression of the interleukin-2 response to recombinant cholera toxin B subunit following vaccination with the live oral cholera vaccine CVD 103-HgR. Infect Immun. 2001;69(3):1574–80. doi:10.1128/IAI.69.3.1574-1580.2001.View ArticlePubMed CentralPubMedGoogle Scholar
- Elias D, Akuffo H, Pawlowski A, Haile M, Schon T, Britton S. Schistosoma mansoni infection reduces the protective efficacy of BCG vaccination against virulent Mycobacterium tuberculosis. Vaccine. 2005;23(11):1326–34. doi:10.1016/j.vaccine.2004.09.038.View ArticlePubMedGoogle Scholar
- Su L, Su CW, Qi Y, Yang G, Zhang M, Cherayil BJ et al. Co-infection with an intestinal helminth impairs host innate immunity against Salmonella and exacerbates intestinal inflammation in mice. Infect Immun. 2014. doi:10.1128/IAI.02023-14Google Scholar
- George PJ, Anuradha R, Kumar NP, Sridhar R, Banurekha VV, Nutman TB, et al. Helminth infections coincident with active pulmonary tuberculosis inhibit mono- and multifunctional CD4+ and CD8+ T cell responses in a process dependent on IL-10. PLoS Pathog. 2014;10(9):e1004375. doi:10.1371/journal.ppat.1004375.View ArticlePubMed CentralPubMedGoogle Scholar
- George PJ, Anuradha R, Kumaran PP, Chandrasekaran V, Nutman TB, Babu S. Modulation of mycobacterial-specific Th1 and Th17 cells in latent tuberculosis by coincident hookworm infection. J Immunol. 2013;190(10):5161–8. doi:10.4049/jimmunol.1203311.View ArticlePubMed CentralPubMedGoogle Scholar
- Walsh KP, Brady MT, Finlay CM, Boon L, Mills KH. Infection with a helminth parasite attenuates autoimmunity through TGF-beta-mediated suppression of Th17 and Th1 responses. J Immunol. 2009;183(3):1577–86. doi:10.4049/jimmunol.0803803.View ArticlePubMedGoogle Scholar
- Elliott DE, Metwali A, Leung J, Setiawan T, Blum AM, Ince MN, et al. Colonization with Heligmosomoides polygyrus suppresses mucosal IL-17 production. J Immunol. 2008;181(4):2414–9.View ArticlePubMed CentralPubMedGoogle Scholar
- Larsson E, Tremaroli V, Lee YS, Koren O, Nookaew I, Fricker A, et al. Analysis of gut microbial regulation of host gene expression along the length of the gut and regulation of gut microbial ecology through MyD88. Gut. 2012;61(8):1124–31. doi:10.1136/gutjnl-2011-301104.View ArticlePubMed CentralPubMedGoogle Scholar
- Upadhyay V, Poroyko V, Kim TJ, Devkota S, Fu S, Liu D, et al. Lymphotoxin regulates commensal responses to enable diet-induced obesity. Nat Immunol. 2012;13(10):947–53. doi:10.1038/ni.2403.View ArticlePubMed CentralPubMedGoogle Scholar
- Qiu J, Guo X, Chen ZM, He L, Sonnenberg GF, Artis D, et al. Group 3 innate lymphoid cells inhibit T-cell-mediated intestinal inflammation through aryl hydrocarbon receptor signaling and regulation of microflora. Immunity. 2013;39(2):386–99. doi:10.1016/j.immuni.2013.08.002.View ArticlePubMedGoogle Scholar
- Shih VF, Cox J, Kljavin NM, Dengler HS, Reichelt M, Kumar P, et al. Homeostatic IL-23 receptor signaling limits Th17 response through IL-22-mediated containment of commensal microbiota. Proc Natl Acad Sci U S A. 2014;111(38):13942–7. doi:10.1073/pnas.1323852111.View ArticlePubMed CentralPubMedGoogle Scholar
- Yang Z, Grinchuk V, Smith A, Qin B, Bohl JA, Sun R, et al. Parasitic nematode-induced modulation of body weight and associated metabolic dysfunction in mouse models of obesity. Infect Immun. 2013;81(6):1905–14. doi:10.1128/IAI.00053-13.View ArticlePubMed CentralPubMedGoogle Scholar
- Morimoto M, Zhao A, Sun R, Stiltz J, Madden KB, Mentink-Kane M, et al. IL-13 receptor alpha2 regulates the immune and functional response to Nippostrongylus brasiliensis infection. J Immunol. 2009;183(3):1934–9. doi:10.4049/jimmunol.0804299.View ArticlePubMed CentralPubMedGoogle Scholar
- Song Y, Garg S, Girotra M, Maddox C, von Rosenvinge EC, Dutta A, et al. Microbiota dynamics in patients treated with fecal microbiota transplantation for recurrent Clostridium difficile infection. PLoS One. 2013;8(11):e81330. doi:10.1371/journal.pone.0081330.View ArticlePubMed CentralPubMedGoogle Scholar
- Barman M, Unold D, Shifley K, Amir E, Hung K, Bos N, et al. Enteric salmonellosis disrupts the microbial ecology of the murine gastrointestinal tract. Infect Immun. 2008;76(3):907–15. doi:10.1128/IAI.01432-07.View ArticlePubMed CentralPubMedGoogle Scholar
- Fadrosh DW, Ma B, Gajer P, Sengamalay N, Ott S, Brotman RM, et al. An improved dual-indexing approach for multiplexed 16S rRNA gene sequencing on the Illumina MiSeq platform. Microbiome. 2014;2(1):6. doi:10.1186/2049-2618-2-6.View ArticlePubMed CentralPubMedGoogle Scholar
- Caporaso JG, Kuczynski J, Stombaugh J, Bittinger K, Bushman FD, Costello EK, et al. QIIME allows analysis of high-throughput community sequencing data. Nat Methods. 2010;7(5):335–6. doi:10.1038/nmeth.f.303.View ArticlePubMed CentralPubMedGoogle Scholar
- White JR, Nagarajan N, Pop M. Statistical methods for detecting differentially abundant features in clinical metagenomic samples. PLoS Comput Biol. 2009;5(4):e1000352. doi:10.1371/journal.pcbi.1000352.View ArticlePubMed CentralPubMedGoogle Scholar