- Research article
- Open Access
Eosinophils may play regionally disparate roles in influencing IgA+ plasma cell numbers during large and small intestinal inflammation
- Ruth Forman1Email author,
- Michael Bramhall1,
- Larisa Logunova1,
- Marcus Svensson-Frej2,
- Sheena M. Cruickshank†1 and
- Kathryn J. Else†1
© The Author(s). 2016
- Received: 15 January 2016
- Accepted: 23 May 2016
- Published: 31 May 2016
Eosinophils are innate immune cells present in the intestine during steady state conditions. An intestinal eosinophilia is a hallmark of many infections and an accumulation of eosinophils is also observed in the intestine during inflammatory disorders. Classically the function of eosinophils has been associated with tissue destruction, due to the release of cytotoxic granule contents. However, recent evidence has demonstrated that the eosinophil plays a more diverse role in the immune system than previously acknowledged, including shaping adaptive immune responses and providing plasma cell survival factors during the steady state. Importantly, it is known that there are regional differences in the underlying immunology of the small and large intestine, but whether there are differences in context of the intestinal eosinophil in the steady state or inflammation is not known.
Our data demonstrates that there are fewer IgA+ plasma cells in the small intestine of eosinophil-deficient ΔdblGATA-1 mice compared to eosinophil-sufficient wild-type mice, with the difference becoming significant post-infection with Toxoplasma gondii. Remarkably, and in complete contrast, the absence of eosinophils in the inflamed large intestine does not impact on IgA+ cell numbers during steady state, and is associated with a significant increase in IgA+ cells post-infection with Trichuris muris compared to wild-type mice. Thus, the intestinal eosinophil appears to be less important in sustaining the IgA+ cell pool in the large intestine compared to the small intestine, and in fact, our data suggests eosinophils play an inhibitory role. The dichotomy in the influence of the eosinophil over small and large intestinal IgA+ cells did not depend on differences in plasma cell growth factors, recruitment potential or proliferation within the different regions of the gastrointestinal tract (GIT).
We demonstrate for the first time that there are regional differences in the requirement of eosinophils for maintaining IgA+ cells between the large and small intestine, which are more pronounced during inflammation. This is an important step towards further delineation of the enigmatic functions of gut-resident eosinophils.
- Plasma cell
- B cell
Eosinophils were originally discovered based on their distinctive “eosin-loving” intracellular granules. These granules contain hydrolytic enzymes and pre-formed cationic granule proteins, including major basic protein (MBP), eosinophil cationic protein (ECP), eosinophil peroxidase (EPO) and eosinophil-derived neurotoxin (EDN). Eosinophils have long been described as end-stage effector cells acting through the secretion of granule-derived proteins, which exert toxic effects on parasites and microbes, but can also cause collateral damage to host tissue cells, especially in allergic inflammation (reviewed [1, 2]). More recently eosinophils have been described as multi-functional leukocytes, acting as sources of numerous cytokines, chemokines, matrix metalloproteinases and reactive oxygen species with a range of functions (reviewed ), in addition to production of eosinophil-specific mediators. Importantly, many, if not all, of the effector molecules are stored within eosinophil-specific granules, allowing for very rapid secretion without the need for de novo synthesis . Alongside the increasing repertoire of eosinophil-derived products there has been an increasing awareness of the broader role eosinophils play in immunity, with a plethora of roles identified for them, including helping shape adaptive immune responses and providing plasma cell survival factors in the bone marrow [5, 6].
Under steady state conditions the gastrointestinal tract (GIT) contains the largest number of eosinophils in the body [7, 8]. Intestinal eosinophils reside primarily in the lamina propria and are important in the maintenance of immune homeostasis in gut-associated tissues . Although the GIT is often considered as a single entity, the large and small intestine are anatomically and functionally different and therefore should be analysed as two separate immunological compartments . In the small intestine there is a higher frequency of eosinophils than in the large intestine  and the eosinophil populations in the large and small intestine are phenotypically different . The functional significance of these phenotypic variants is however not known, although the increased frequency of eosinophils in the small versus large intestine implies they may be of greater functional significance in this region of the GIT, at least in the steady state.
Despite the literature describing differences in the number and phenotype of eosinophils in the naïve small and large intestine, and a functional role for the eosinophil in supporting plasma cells during steady state conditions, it is not known whether the small intestinal eosinophil has unique functions compared to the large intestinal eosinophil and whether this is altered during inflammation. Eosinophilia is observed in response to infection and during inflammation of both the large [13, 14] and small intestine , and virtually any inflammatory condition of the GIT can feature an eosinophilia. Thus, eosinophils are not simply indicative of a Th2 disorder, but rather can be prominent in many diverse inflammatory conditions. Indeed, a number of human and translational studies have shown that eosinophils are increased in intestinal tissues affected by inflammatory bowel disease . Here we use two models of parasitic infection – chronic Trichuris muris  infection and Toxoplasma gondii infection, that drive an inflammatory response in the GIT restricted to the large and small intestine, respectively. Thus use of these two complementary infection models allows a dissection of the functional roles of the eosinophil in the context of the IgA+ cells in both the large intestine and small intestine.
T. muris and T. gondii infections drive eosinophilia in the large and small intestine
IgA expression during T. gondii infection
IgA expression during T. muris infection
IgA expression during T. gondii RH infection
Having confirmed regional differences in the importance of the eosinophil in sustaining IgA+ plasma cells using the same parasitic infection (T. gondii RH), all subsequent experiments utilised low dose T. muris infections for analyses of the large intestine and T. gondii PRU infections for analyses of the small intestine, respectively. Although infection with T. gondii RH allowed simultaneous analysis of both the small and large intestine, the more virulent infection was associated with higher morbidity and therefore not utilised in further experiments.
Plasma cell survival, recruitment factors and proliferation during T. muris and T. gondii infection
Finally, to determine if the effect of eosinophil-deficiency on plasma cell numbers is due to altered local plasma cell proliferation, co-staining for Ki67 and IgA was performed on GIT sections from the small intestine of naïve and T. gondii-infected mice by double immunofluorescence. In both naïve and infected ΔdblGATA-1 and wild-type mice, no proliferating IgA+ plasma cells (Fig. 6i; IgA+Ki67+) were observed in any of the stained sections, suggesting that the lamina propria-resident plasma cells do not proliferate in situ.
Eosinophils are a major cellular component of the gastrointestinal tract and following parasitic infection the number of eosinophils is significantly increased. While historically being viewed as end-stage effector cells, the eosinophil is increasingly recognised as a cell type that interacts with cells of both the innate and adaptive immune system. For example, the generation and maintenance of IgA+ plasma cells is dependent on eosinophils [5, 6, 9]. Previous work has reported a reduction in the number of IgA+ plasma cells in both the small and large intestine of eosinophil-deficient mice under steady state conditions , although no statistical significance was ascribed to these changes. In keeping with this report we see a non-significant decrease in IgA+ plasma cells in the small intestine of eosinophil-deficient mice under steady state conditions, while the number of IgA+ plasma cells were equivalent in the uninfected large intestine in the presence or absence of eosinophils.
Importantly, we show for the first time that eosinophils play distinct roles in supporting IgA+ plasma cells following infection-driven intestinal inflammation, depending on the gastrointestinal tract niche they occupy. In the large intestine, eosinophil-deficient mice have a significant increase in plasma cells compared to wild-type mice, whereas in the small intestine plasma cell numbers are significantly lower in eosinophil-deficient mice compared to infected wild-type mice. Our data thus demonstrates a relative dependency of plasma cells on eosinophils according to the intestinal niche, and suggests that there is a critical role for eosinophils in maintaining plasma cells in the small but not large intestine. The regional differences in the requirement for eosinophils in maintaining IgA+ plasma cells is an important and novel observation, suggesting that the enigmatic functions of the intestinal eosinophil may differ according to intestinal niche, and with this data further emphasising that the two compartments of the gut are distinct and that findings from one should not be extrapolated to the other.
Eosinophils have been identified as a key producer of plasma cell survival factors in the bone marrow [5, 6]. However, it was recently reported that the role of eosinophils in maintaining plasma cells in the intestine appears to be independent of eosinophil-derived APRIL and BAFF . In keeping with this recent publication, our analysis of intestinal tissue revealed no major differences in the plasma cell survival factors APRIL, BAFF, IL-6 or GM-CSF between eosinophil-deficient and control mice following infection. Therefore, although gastrointestinal eosinophils may be capable of producing these survival factors , they are not the key source of these factors and other intestinal cells, including epithelial cells , T cells and dendritic cells  may compensate for the absence of eosinophils. Furthermore, we also assessed whether the differences in IgA+ plasma cell frequencies could be attributed to either recruitment or proliferation. Both MAdCAM-1 and CCL25 have previously been suggested to be important in the recruitment of plasma cells to the intestine [19, 20]; therefore the expression of these molecules in eosinophil-deficient and control mice post-infection was analysed. However, our data suggests that differences in MAdCAM-1 or CCL25 expression do not underlie the different phenotypes observed in the small and large intestine in the absence of eosinophils. Moreover, we detected no IgA+ plasma cell proliferation within the lamina propria of the small intestine in either the ΔdblGATA-1 or control mice, neither at baseline nor post-infection with T. gondii, suggesting that the differences observed in plasma cell numbers is not due to altered proliferation of these cells in the intestinal tissue. This is in agreement with previously published data that shows the majority of plasma cells do not divide within the intestinal lamina propria in C57BL/6 mice .
One potential candidate driving differential IgA+ phenotypes in the small and large intestine is the microbiota, with the abundance and composition of the microbiota being markedly different in the small versus large intestine . The gut microbiota is known to be important in driving mucosal T cell-independent induction of secretory IgA within the lamina propria . Recently it was reported that the intestinal milieu contributes to the expression of unique niche-dependent transcripts by eosinophils. For example, CD22 is highly expressed on upper GI tract eosinophils, but present at significantly lower levels by eosinophils in other areas of the gut, with colonic eosinophils having the lowest expression levels . Moreover, the duodenum and jejunum are particularly enriched for eosinophils that express ST2, CD69, Ly6C and CD11c . These differences may infer the existence of different subpopulations of eosinophils, with unique functions at different niches throughout the intestine. Therefore, the absence of eosinophils in the small intestine could result in a different effect on plasma cell numbers compared to a deficiency in the large intestinal eosinophil. For example, in niches where eosinophils are rare and appear to be less activated, e.g. expressing lower levels of CD11c, such as the colon , there may be a lower dependence on the eosinophil for maintenance of plasma cell numbers with other cell types taking a more prominent role. Again this further emphasises the need for focused regional dissections of immune function along the GIT.
In conclusion, we show for the first time the impact of eosinophil-deficiency on IgA+ plasma cells numbers during inflammation in the small and large intestine. We demonstrate that eosinophils appear to be crucial for the maintenance and/or generation of IgA+ cells in the small intestine lamina propria post-infection. In complete contrast, the absence of eosinophils in the inflamed large intestine results in an increase in IgA+ cells. Therefore, the role of eosinophils appears to be dependent upon the region of the GIT in which they reside, and this is even more pronounced during inflammation, perhaps reflective of the greater need for restoration of the IgA barrier function.
Animals, T. muris and T. gondii
BALB/c mice were purchased from Harlan U.K. (Bicester, U.K.). ΔdblGATA-1 mice on a BALB/c background were bred in-house. Male mice were used for all experiments. For T. muris infections mice were infected with 20 infective T. muris eggs when 8 –10 weeks old and sacrificed at various time points after infection. The maintenance of T. muris and the method of infection were as previously described , worm burden in the large intestine was assessed as previously described . Tachyzoites of the type I eYFP expressing RH and the tandem dimeric tomato RFP- tagged type II Pruginaud (PRU) strains of Toxoplasma gondii, from Boris Striepen , were maintained by serial passage through confluent monolayers of human foreskin fibroblasts . Mice were infected by oral gavage with 106 RH or PRU tachyzoites and sacrificed at various time points post infection by exposure to carbon dioxide gas in a rising concentration. In order to ameliorate animal suffering mice were regularly weighed during infection and general appearance monitored, if any mice lost more than 20 % bodyweight they were humanely killed. All animal experiments were approved by the University of Manchester Animal Welfare and Ethical Review Board and performed under the regulation of the Home Office Scientific Procedures Act (1986) and the Home Office approved grant 40/3217.
Extraction of total RNA and reverse transcription
Tissue samples from the junction of the caecum and large intestine, jejunum or brain were placed in TRIsure (Bioline, London, UK) and frozen on dry ice. Samples were homogenised using a FastPrep 24 and lysing matrix D (MP Biomedicals, Illkirch, France) and total RNA extracted according to the manufacturer’s instructions for TRIsure. Resulting RNA was quantified on a Nanodrop ND-1000 spectrophotometer (Labtech International, East Sussex, U.K.) and stored at −80 °C until used. 1.0 μg of RNA was treated with RNase-free DNase (Promega, Southampton, UK) and reverse transcribed using BioScript (Bioline) in a final volume of 30 μl according to the manufacturer’s instructions and stored at -20 °C.
Quantitative PCR on intestinal tissue
Quantitative PCR for T. gondii parasite burden
Parasite burden was assessed as previously described . Briefly, Quantitative PCR was performed using KAPA SYBR FAST qPCR kit (KapaBiosystems) on a BioRad MyQ2 Cycler with Optical System software version 2.1. Relative mRNA levels were calculated for toxoplasma cysts (Forward: CGTTTGGAGAAATGGTGTCCCAG; Reverse: CCGCCTGAGTATCCGCTTTTAC) by using an included standard curve for each individual gene and normalised to the housekeeping gene TBP (Forward: AACAGCAGCAGCAACAACAGCAGG; Reverse: TGATAGGGGTCATAGGAGTCATTGG).
Histological sections were prepared from proximal large intestine or jejunum and preserved in OCT. 6-μm sections were cut using a microtome and placed on polysine adhesion slides. Immunohistochemical staining for IgA was performed as follows. Slides were fixed in 4 % PFA on ice for 10 mins. Endogenous peroxidase was quenched by incubation with 1.5 U/ml glucose oxidase (Sigma, Gillingham, Dorset, U.K.) in the presence of 1.8 mg/ml glucose and 0.064 mg/ml sodium azide for 20 min at 37 °C. Non-specific binding was blocked with 7 % rat serum (Sigma) and endogenous avidin and biotin binding sites were blocked using a kit according to the manufacturer’s instructions (Invitrogen, Paisley, UK). Sections were then incubated with biotinylated rat anti-mouse IgA (5 μg/ml, BD Biosciences) in phosphate-buffered saline, followed by ABC (avidin-biotin complex) (Vector Laboratories) and 3,3′ Diaminobenzidine (DAB; Vector) and colour development monitored. Sections were counter-stained in HaemQS (Vector Laboratories) for 1 min, and mounted in aquamount (BDH, Lutterworth, UK). For MAdCAM-1 and Siglec F staining the same protocol was used but non-specific binding sites were blocked with 7 % goat serum (Invitrogen), a MAdCAM-1 (5 μg/ml, eBiosciences) or Siglec F primary antibody (5 μg/ml, BD Biosciences) was used followed by a biotinylated secondary goat anti rat Fab’ fragment antibody (1 μg/ml, Santa Cruz). For IgA staining 0.05 % Saponin was utilised in all washing and staining steps.
Slides were blinded and positive cells counted in a minimum of 20 crypts or 10 VCUs from 3 sections evenly distributed across the specimen. Images were acquired using a 20×/0.80 Plan Apo objective using the 3D Histech Pannoramic 250 Flash II slide scanner. Isotype control staining was performed and examined to confirm there was no non-specific staining (Additional file 1: Figure S1).
Histological sections were prepared from proximal large intestine or jejunum and preserved in OCT. 6-μm sections were cut using a microtome and placed on polysine adhesion slides. Slides were fixed in 4 % paraformaldehyde at 4 °C for 10 min. Sections were blocked using the tyramide blocking kit (PerkinElmer, Cambridge, UK) for 30 min. Endogenous biotins were blocked using the avidin/biotin blocking kit as per the manufacturer’s instructions (Invitrogen). Slides were first stained with biotinylated rat anti-mouse IgA (5 μg/ml, BD Biosciences), followed by a secondary avidin Texas-Red (Vector Lab, 30μg/ml). Slides were then incubated with the primary antibody Ki67-Alexa Flour® 488 (5μg/ml, BD Biosciences). Slides were washed and mounted with vector shield containing 4’,6-diamidino-2-phenylindole (Vector Lab). 0.05 % Saponin was utilised in all washing and staining steps.
The proportion of PCs in the MLN was assessed by flow cytometry. Single cell suspensions were incubated with Fc block prior to staining with Biotinylated-B220 or FITC-B220 and APC-CD138 (BD Biosciences) and subsequently Streptavidin-QDOT605 (Invitrogen). Samples were acquired using an LSRII (BD Biosciences) and data were analysed with FACSDiva (BD Biosciences) and FlowJo 10 (Tree Star).
Statistical analysis was performed using the Student’s t test or 2 WAY ANOVA with post-hoc Bonferonni’s test, as appropriate with the statistical package GraphPad Prism 6.04 (GraphPad Software, San Diego, U.S.A.). A probability value of <0.05 was considered significant (*p < 0.05, **p < 0.01, ***p < 0.001).
ECP, Eosinophil cationic protein; EDN, Eosinophil-derived neurotoxin; EPO, Eosinophil peroxidase; GIT, gastrointestinal tract; MBP, major nasic protein; MLN, mesenteric lymph node; NS, Not significant; PRU, Pruginaud; T. gondii, Toxoplasma gondii; T. muris, Trichuris muris
The Bioimaging Facility microscopes used in this study were purchased with grants from BBSRC, Wellcome and the University of Manchester Strategic Fund.
The work was supported by a Wellcome Trust grant number 092323.
Availability of data and materials
The datasets supporting the conclusions of this article are included within the article and its supplemental file.
RF was involved in study design, performed experiments and data analysis and wrote the manuscript. LL performed qPCR analysis, fluorescent microscopy and did some data analysis. MB performed one of the Pru experiments and did data analysis. KJE, SMC and MSF conceived of the study, participated in its design and coordination, and helped to draft the manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Consent for publication
Ethics approval and consent to participate
All animal experiments were approved by the University of Manchester Animal Welfare and Ethical Review Board and performed under the regulation of the Home Office Scientific Procedures Act (1986) and the Home Office approved grant 40/3217.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- Acharya KR, Ackerman SJ. Eosinophil granule proteins: form and function. J Biol Chem. 2014;289(25):17406–15.View ArticlePubMedPubMed CentralGoogle Scholar
- Jones DG. The eosinophil. J Comp Pathol. 1993;108(4):317–35.View ArticlePubMedGoogle Scholar
- Davoine F, Lacy P. Eosinophil cytokines, chemokines, and growth factors: emerging roles in immunity. Front Immunol. 2014;5:570.View ArticlePubMedPubMed CentralGoogle Scholar
- Beil WJ, Weller PF, Tzizik DM, Galli SJ, Dvorak AM. Ultrastructural immunogold localization of tumor necrosis factor-alpha to the matrix compartment of eosinophil secondary granules in patients with idiopathic hypereosinophilic syndrome. J Histochem Cytochem. 1993;41(11):1611–5.View ArticlePubMedGoogle Scholar
- Chu VT, Berek C. Immunization induces activation of bone marrow eosinophils required for plasma cell survival. Eur J Immunol. 2012;42(1):130–7.View ArticlePubMedGoogle Scholar
- Chu VT, Frohlich A, Steinhauser G, Scheel T, Roch T, Fillatreau S, Lee JJ, Lohning M, Berek C. Eosinophils are required for the maintenance of plasma cells in the bone marrow. Nat Immunol. 2011;12(2):151–9.View ArticlePubMedGoogle Scholar
- Powell N, Walker MM, Talley NJ. Gastrointestinal eosinophils in health, disease and functional disorders. Nat Rev Gastroenterol Hepatol. 2010;7(3):146–56.View ArticlePubMedGoogle Scholar
- Zuo L, Rothenberg ME. Gastrointestinal eosinophilia. Immunol Allergy Clin North Am. 2007;27(3):443–55.View ArticlePubMedPubMed CentralGoogle Scholar
- Chu VT, Beller A, Rausch S, Strandmark J, Zanker M, Arbach O, Kruglov A, Berek C. Eosinophils promote generation and maintenance of immunoglobulin-a-expressing plasma cells and contribute to gut immune homeostasis. Immunity. 2014;40(4):582–93.View ArticlePubMedGoogle Scholar
- Bowcutt R, Forman R, Glymenaki M, Carding SR, Else KJ, Cruickshank SM. Heterogeneity across the murine small and large intestine. World J Gastroenterol. 2014;20(41):15216–32.View ArticlePubMedPubMed CentralGoogle Scholar
- Mishra A, Hogan SP, Lee JJ, Foster PS, Rothenberg ME. Fundamental signals that regulate eosinophil homing to the gastrointestinal tract. J Clin Invest. 1999;103(12):1719–27.View ArticlePubMedPubMed CentralGoogle Scholar
- Wen T, Mingler MK, Blanchard C, Wahl B, Pabst O, Rothenberg ME. The pan-B cell marker CD22 is expressed on gastrointestinal eosinophils and negatively regulates tissue eosinophilia. J Immunol. 2012;188(3):1075–82.View ArticlePubMedPubMed CentralGoogle Scholar
- Svensson M, Bell L, Little MC, DeSchoolmeester M, Locksley RM, Else KJ. Accumulation of eosinophils in intestine-draining mesenteric lymph nodes occurs after Trichuris muris infection. Parasite Immunol. 2011;33(1):1–11.View ArticlePubMedPubMed CentralGoogle Scholar
- Woodruff SA, Masterson JC, Fillon S, Robinson ZD, Furuta GT. Role of eosinophils in inflammatory bowel and gastrointestinal diseases. J Pediatr Gastroenterol Nutr. 2011;52(6):650–61.View ArticlePubMedGoogle Scholar
- Hogan SP, Mishra A, Brandt EB, Foster PS, Rothenberg ME. A critical role for eotaxin in experimental oral antigen-induced eosinophilic gastrointestinal allergy. Proc Natl Acad Sci U S A. 2000;97(12):6681–6.View ArticlePubMedPubMed CentralGoogle Scholar
- Bancroft AJ, Else KJ, Grencis RK. Low-level infection with Trichuris muris significantly affects the polarization of the CD4 response. Eur J Immunol. 1994;24(12):3113–8.View ArticlePubMedGoogle Scholar
- Zhang JQ, Biedermann B, Nitschke L, Crocker PR. The murine inhibitory receptor mSiglec-E is expressed broadly on cells of the innate immune system whereas mSiglec-F is restricted to eosinophils. Eur J Immunol. 2004;34(4):1175–84.View ArticlePubMedGoogle Scholar
- Yu C, Cantor AB, Yang H, Browne C, Wells RA, Fujiwara Y, Orkin SH. Targeted deletion of a high-affinity GATA-binding site in the GATA-1 promoter leads to selective loss of the eosinophil lineage in vivo. J Exp Med. 2002;195(11):1387–95.View ArticlePubMedPubMed CentralGoogle Scholar
- Schippers A, Leuker C, Pabst O, Kochut A, Prochnow B, Gruber AD, Leung E, Krissansen GW, Wagner N, Muller W. Mucosal addressin cell-adhesion molecule-1 controls plasma-cell migration and function in the small intestine of mice. Gastroenterology. 2009;137(3):924–33.View ArticlePubMedGoogle Scholar
- Bowman EP, Kuklin NA, Youngman KR, Lazarus NH, Kunkel EJ, Pan J, Greenberg HB, Butcher EC. The intestinal chemokine thymus-expressed chemokine (CCL25) attracts IgA antibody-secreting cells. J Exp Med. 2002;195(2):269–75.View ArticlePubMedPubMed CentralGoogle Scholar
- Jung Y, Wen T, Mingler MK, Caldwell JM, Wang YH, Chaplin DD, Lee EH, Jang MH, Woo SY, Seoh JY, et al. IL-1beta in eosinophil-mediated small intestinal homeostasis and IgA production. Mucosal Immunol. 2015;8(4):930–42.View ArticlePubMedPubMed CentralGoogle Scholar
- He B, Xu W, Santini PA, Polydorides AD, Chiu A, Estrella J, Shan M, Chadburn A, Villanacci V, Plebani A, et al. Intestinal bacteria trigger T cell-independent immunoglobulin A(2) class switching by inducing epithelial-cell secretion of the cytokine APRIL. Immunity. 2007;26(6):812–26.View ArticlePubMedGoogle Scholar
- Schneider P, MacKay F, Steiner V, Hofmann K, Bodmer JL, Holler N, Ambrose C, Lawton P, Bixler S, Acha-Orbea H, et al. BAFF, a novel ligand of the tumor necrosis factor family, stimulates B cell growth. J Exp Med. 1999;189(11):1747–56.View ArticlePubMedPubMed CentralGoogle Scholar
- Mesin L, Di Niro R, Thompson KM, Lundin KE, Sollid LM. Long-lived plasma cells from human small intestine biopsies secrete immunoglobulins for many weeks in vitro. J Immunol. 2011;187(6):2867–74.View ArticlePubMedGoogle Scholar
- Macpherson AJ, Gatto D, Sainsbury E, Harriman GR, Hengartner H, Zinkernagel RM. A Primitive T Cell-Independent Mechanism of Intestinal Mucosal IgA Responses to Commensal Bacteria. Science. 2000;288(5474):2222–6.View ArticlePubMedGoogle Scholar
- Chu DK, Jimenez-Saiz R, Verschoor CP, Walker TD, Goncharova S, Llop-Guevara A, Shen P, Gordon ME, Barra NG, Bassett JD, et al. Indigenous enteric eosinophils control DCs to initiate a primary Th2 immune response in vivo. J Exp Med. 2014;211(8):1657–72.View ArticlePubMedPubMed CentralGoogle Scholar
- Wakelin D. Acquired immunity to Trichuris muris in the albino laboratory mouse. Parasitology. 1967;57(3):515–24.View ArticlePubMedGoogle Scholar
- Else KJ, Wakelin D, Wassom DL, Hauda KM. The influence of genes mapping within the major histocompatibility complex on resistance to Trichuris muris infections in mice. Parasitology. 1990;101(Pt 1):61–7.View ArticlePubMedGoogle Scholar
- Schaeffer M, Han SJ, Chtanova T, van Dooren GG, Herzmark P, Chen Y, Roysam B, Striepen B, Robey EA. Dynamic imaging of T cell-parasite interactions in the brains of mice chronically infected with Toxoplasma gondii. J Immunol. 2009;182(10):6379–93.View ArticlePubMedGoogle Scholar
- Egan CE, Dalton JE, Andrew EM, Smith JE, Gubbels MJ, Striepen B, Carding SR. A requirement for the Vgamma1+ subset of peripheral gammadelta T cells in the control of the systemic growth of Toxoplasma gondii and infection-induced pathology. J Immunol. 2005;175(12):8191–9.View ArticlePubMedGoogle Scholar
- Jones LA, Roberts F, Nickdel MB, Brombacher F, McKenzie AN, Henriquez FL, Alexander J, Roberts CW. IL-33 receptor (T1/ST2) signalling is necessary to prevent the development of encephalitis in mice infected with Toxoplasma gondii. Eur J Immunol. 2010;40(2):426–36.View ArticlePubMedGoogle Scholar