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Open Access

Peer-reviewed

Research Article

Impaired Cellular Immunity in the Murine Neural Crest Conditional Deletion of Endothelin Receptor-B Model of Hirschsprung’s Disease

  • Ankush Gosain ,

    gosain@surgery.wisc.edu

    Affiliations Department of Surgery, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America, Department of Neuroscience, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America

    ⨯
  • Amanda J. Barlow-Anacker,

    Affiliation Department of Surgery, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America

    ⨯
  • Chris S. Erickson,

    Affiliation Department of Surgery, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America

    ⨯
  • Joseph F. Pierre,

    Affiliation Department of Surgery, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America

    ⨯
  • Aaron F. Heneghan,

    Affiliation Department of Surgery, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America

    ⨯
  • Miles L. Epstein,

    Affiliation Department of Neuroscience, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America

    ⨯
  • Kenneth A. Kudsk

    Affiliations Department of Surgery, University of Wisconsin-Madison School of Medicine and Public Health, Madison, Wisconsin, United States of America, Veteran Administration Surgical Service, William S. Middleton Memorial Veterans Hospital, Madison, United States of America

    ⨯

Abstract

Hirschsprung’s disease (HSCR) is characterized by aganglionosis from failure of neural crest cell (NCC) migration to the distal hindgut. Up to 40% of HSCR patients suffer Hirschsprung’s-associated enterocolitis (HAEC), with an incidence that is unchanged from the pre-operative to the post-operative state. Recent reports indicate that signaling pathways involved in NCC migration may also be involved in the development of secondary lymphoid organs. We hypothesize that gastrointestinal (GI) mucosal immune defects occur in HSCR that may contribute to enterocolitis. EdnrB was deleted from the neural crest (EdnrBNCC-/-) resulting in mutants with defective NCC migration, distal colonic aganglionosis and the development of enterocolitis. The mucosal immune apparatus of these mice was interrogated at post-natal day (P) 21–24, prior to histological signs of enterocolitis. We found that EdnrBNCC-/- display lymphopenia of their Peyer’s Patches, the major inductive site of GI mucosal immunity. EdnrBNCC-/- Peyer’s Patches demonstrate decreased B-lymphocytes, specifically IgM+IgDhi (Mature) B-lymphocytes, which are normally activated and produce IgA following antigen presentation. EdnrBNCC-/- animals demonstrate decreased small intestinal secretory IgA, but unchanged nasal and bronchial airway secretory IgA, indicating a gut-specific defect in IgA production or secretion. In the spleen, which is the primary source of IgA-producing Mature B-lymphocytes, EdnrBNCC-/- animals display decreased B-lymphocytes, but an increase in Mature B-lymphocytes. EdnrBNCC-/- spleens are also small and show altered architecture, with decreased red pulp and a paucity of B-lymphocytes in the germinal centers and marginal zone. Taken together, these findings suggest impaired GI mucosal immunity in EdnrBNCC-/- animals, with the spleen as a potential site of the defect. These findings build upon the growing body of literature that suggests that intestinal defects in HSCR are not restricted to the aganglionic colon but extend proximally, even into the ganglionated small intestine and immune cells.

Citation: Gosain A, Barlow-Anacker AJ, Erickson CS, Pierre JF, Heneghan AF, Epstein ML, et al. (2015) Impaired Cellular Immunity in the Murine Neural Crest Conditional Deletion of Endothelin Receptor-B Model of Hirschsprung’s Disease. PLoS ONE 10(6): e0128822. https://doi.org/10.1371/journal.pone.0128822

Academic Editor: Anatoly V. Grishin, Childrens Hospital Los Angeles, UNITED STATES

Received: November 12, 2014; Accepted: May 1, 2015; Published: June 10, 2015

This is an open access article, free of all copyright, and may be freely reproduced, distributed, transmitted, modified, built upon, or otherwise used by anyone for any lawful purpose. The work is made available under the Creative Commons CC0 public domain dedication

Data Availability: All relevant data are within the paper and its Supporting Information files.

Funding: This work was supported by the National Institutes of Health (NIDDK RO1DK081634) to MLE, the Veteran’s Affairs Office of Research and Development (Biomedical Laboratory Research & Development Award I01BX001672) to KAK, the Central Surgical Association Foundation (2012 Turcotte Award) to AG, the American Pediatric Surgical Association Foundation Award to AG, and the National Institutes of Health (NIDDK K08DK098271) to AG. The contents of this article do not represent the views of the Veterans Affairs or the United States Government (KAK).

Competing interests: The authors have declared that no competing interests exist.

Introduction

Hirschsprung’s disease (HSCR, Online Mendelian Inheritence in Man #142623) is a common cause of intestinal obstruction in the newborn and is characterized by an absence of enteric nervous system (ENS) ganglion cells in the distal hindgut, extending from the rectum to a variable distance proximally. Failure of cranial-caudal neural crest cell (NCC) migration results in an aganglionic segment that exhibits tonic contraction, causing a functional bowel obstruction [1,2]. Untreated, this leads to progressive bowel distention, the development of Hirschsprung’s-associated enterocolitis (HAEC), and death. HAEC is a significant and potentially life-threatening complication of HSCR [3,4], with an incidence that ranges from 20–58% and carries a mortality of 2.5–9%, accounting for the majority of deaths from HSCR [5,6]. While HSCR is traditionally treated with surgical resection of the aganglionic segment and “pull-through” of ganglionated bowel to the anus, the incidence of HAEC appears to be unchanged from the pre-operative to post-operative state in both animals and humans [7–9], suggesting bowel obstruction is not the sole etiology. However, the precise etiology of HAEC remains elusive.

HAEC occurs in two forms, pre-operative (or neonatal) and post-operative [10–12]. Factors thought to contribute to the pathogenesis in both forms include abnormal goblet cell function, decreased secretory immunoglobulin A (SIgA) secretion, and leukocyte dysfunction[3,4,13]. Additionally, multiple investigators have postulated that HAEC develops in the setting of distal bowel obstruction[14] and have demonstrated similar histopathologic changes in experimental models of bowel obstruction to those in HAEC-affected bowel, including polymorphonuclear cell infiltration and mucous retention within the intestinal crypts, and the development of crypt abscesses[15]. However, while animal models of distal bowel obstruction share findings of focal inflammation and the development of punctate ulcers, they do not demonstrate the excessive mucous production or crypt abscesses that are found in HAEC [16]. Additionally, the clinical observation of continued susceptibility to HAEC in the post-pull-through period argues against obstruction as the sole etiology. Furthermore, investigations into an infectious cause for HAEC have failed to identify a single, responsible organism [17,18]. However, recent studies in mouse models of HSCR/HAEC have identified broader changes in the intestinal microbiome that may contribute to HAEC[19,20].

Multiple genetic defects have been associated with HSCR and failure of NCC migration, most commonly mutations of Rearranged during transfection (Ret) and of Endothelin receptor B (EdnrB)[1,21–27]. RET encodes a transmembrane receptor kinase, that binds a complex of the ligand Glial cell Derived Neurotrophic Factor (GDNF) and its receptor GDNF Family Receptor α (GFRα), thereby stimulating NCC survival, proliferation, migration and differentiation[28]. Ret has additionally been identified as necessary for the development of Peyer’s patches (PP)[29], the primary inductive site for gastrointestinal (GI) host defense[30], providing further evidence for a potential developmental link between the ENS and GI mucosal immunity. Unfortunately, RET knockout animals exhibit a severe phenotype with NCC colonization limited to the esophagus and stomach and renal agenesis[31]. These animals die shortly after birth, making them unsuitable for the study of post-natal HAEC[31].

EdnrB and its ligand, endothelin 3 (ET3), regulate NCC proliferation, migration and differentiation[32,33]. Naturally occurring mutations of both EdnrB and ET3 have been found in mice; the piebald lethal strain lacks EdnrB and the lethal spotted strain lacks ET3[34,35]. Experimental mutation of EdnrB results in aganglionosis of the distal hindgut, mimicking that seen in the piebald lethal and lethal spotted strains as well as the common clinical finding in HSCR patients[36,37]. We have developed and characterized mice with a conditional neural crest-specific deletion of EdnrB (EdnrBNCC-/-)[37]. These mice exhibit distal colonic aganglionosis and develop HAEC, closely modeling human HSCR and HAEC[19,38,39]. We have recently described the time course of development of HAEC, alterations in the colonic microbiota, and impaired innate immune function in these animals[19].

Here, we used the NCC deletion of EdnrB (EdnrBNCC-/-) model of HSCR and HAEC to systematically examine the GI mucosal immune apparatus and its potential contribution to the development of HAEC. Prior to histological signs of enterocolitis, we find that EdnrBNCC-/- animals demonstrate a gut-specific deficiency in secretory IgA. These mice have small, lymphopenic PP with reduced mature B-lymphocytes. Interestingly, they also show increased mature B-lymphocytes in the spleen, the primary source of this cell population. Our findings suggest impaired cellular immunity may contribute to the development of HAEC.

Materials and Methods

Ethics Statement

All procedures were approved by the University of Wisconsin Institutional Animal Care and Use Committee (Protocol #M01392).

Animals

We utilized a mouse model with NCC deletion of Endothelin Receptor B (EdnrBflex3/flex3)[37]. Mating TgWnt1-Cre/+;EdnrBflex3/+ mice with Rosa26floxStop/tdTomato;EdnrBflex3/flex3 mice resulted in either heterozygous (EdnrBflex3/+) or homozygous deletion of EdnrB (EdnrBflex3/flex3), (defined throughout the manuscript as EdnrBNCC+/- and EdnrBNCC-/-, respectively). In addition, NCC in these mice express tdTomato [39]. Mice were housed in a non-sterile environment and were allowed ad libitum access to standard rodent chow and water. EdnrBNCC+/- animals were utilized as littermate controls. EdnrBNCC+/- mice are available from Jackson Laboratories (Stock Number: 009063).

Immunohistochemistry and Scoring for Enterocolitis

Tissue sections were either fixed in 4% formalin, processed (Tissue-Tek V.I.P), and embedded in paraffin or fixed in 4% paraformaldehyde and processed into 30% sucrose prior to sectioning. Segments of colon and ileum were harvested from EdnrBNCC+/- and EdnrBNCC-/- animals at P21-24 and P26-29 (n = 4–6 animals per group, per time point). Fresh specimens were fixed in 4% paraformaldehyde for 24 hours and submitted to the University of Wisconsin Department of Surgery Histology Core for further processing into paraffin blocks. Paraffin-embedded small intestine and colon specimens were sectioned at a thickness of 5 microns, deparaffinized in xylene and stained with routine hematoxylin & eosin (H&E), as previously described [19]. H&E-stained sections were scored for severity and depth of inflammation by blinded observers from the Department of Pathology using the semi-quantitative Murine Enterocolitis Grading System developed by Cheng, et.al.[40].

Paraffin tissue sections of PP were stained for T cells (CD3, M7254, 1:100, Rabbit anti-human polyclonal antibody, Dako) and B cells (CD45R/B220, 1:50, Rat anti-mouse polyclonal antibody, cat. 550286 BD Biosystems, San Jose, CA) and visualized with goat anti-rat IgG secondary antibody (Alexa Fluor 488, 1:500, Invitrogen, Carlsbad, CA) and goat anti-rabbit IgG secondary antibody (Alexa Fluor 568, 1:500, Invitrogen), respectively. Sections were counter-stained with DAPI solution (P36935, Invitrogen). 16μm cryosections of spleen were stained in a similar manner with CD3, B220 and MOMA (1:400, anti-rabbit biotin, ab51813, Abcam) and visualized with goat anti-rabbit Alexa Fluor 647, goat anti-rat Alexa Fluor 488 and streptavidin conjugated 568 (Invitrogen), respectively.

Slides were imaged on a Nikon A1 confocal microscope. Z-series were captured, processed, and analyzed with Nikon Elements (Nikon, Melville, NY, USA). The brightness and contrast may have been adjusted using Photoshop (Adobe systems, New York, NY).

Isolation of Lymphocytes

After euthanasia, 500μL of blood was collected by cardiac puncture. Blood samples were diluted to 4mL with HBSS (Lonza, Walkersville, MD) and Ficoll-Paque (GE Healthcare, Precataway, NJ) separation used to obtain the lymphocyte layer.

The peritoneal cavity was opened and the small intestine (SI) isolated and flushed with 10mL of cold CMF-HBSS containing 50000U penicillin and 50mg/mL streptomycin (Sigma, St. Louis, MO). PP were removed from the entire length of the SI and placed into 1.5mL tubes of CMF-HBSS. PP were strained through 100μm mesh with a total volume of 15mL CMF-HBSS. The effluent was collected and spun at 1000rpm at 4°C for 10 minutes. Supernatant was removed and the pellet re-suspended in 2mL of 1xPBS containing 0.5% bovine serum albumin (BSA) and stored on ice.

The spleen was removed from the peritoneal cavity and strained through a 40μm nylon mesh filter. The cell suspension was transferred to a 15mL tube which was spun at 1000rpm for 10 minutes at 4°C. The supernatant was discarded and the pellet was re-suspended in 5mL of 1X Lysis buffer (PharM Lyse, Becton-Dickinson, Franklin Lakes, NJ). This was incubated for 15 minutes at room temperature (RT) protected from light. The tube was then spun at 1000rpm for 10 minutes at 4°C. The supernatant was discarded and the pellet re-suspended with 2mL 1xPBS containing 0.5% BSA.

To isolate bone marrow lymphocytes, the femur was removed and the tips excised. The bone was flushed with CMF-HBSS via syringe with a 27 gauge needle and bone marrow cells filtered through a 40μm nylon mesh filter. Red blood cells were removed by incubation with Lysis buffer, as described above.

Cells were counted by Trypan blue exclusion on a hemocytometer and recorded. For flow cytometry, the cell density was adjusted to approximately 1x106 cells/mL with staining buffer (Becton-Dickinson, Franklin Lakes, NJ) prior to antibody staining.

Flow Cytometry Analysis

75μL of the cell solution (1x106 cells/mL) was added to a clean 15mL tube (Falcon 2058) in duplicate with 10μL of respective antibody solution (T or B cell antibody solution). The T cell antibody solution contained the following fluorochrome conjugated antibodies from BD Pharmingen (San Diego, CA) at a final concentration of 2.5μg/mL in staining buffer: Pacific Blue-conjugated mAb to CD3 (145-2C11), Alexa 700-conjugated mAb to CD4 (RM4-5), PerCP-Cy5.5-conjugated mAb to CD8a (53–6.7), APC-Alexa fluor 750 mAB to L-selectin (Ly-22). The B cell antibody solution contained the following fluorochrome-conjugated antibodies from BD Pharmingen at a final concentration of 2.5μg/mL: Pacific Blue-conjugated mAb to CD3 (145-2C11), Alexa 700-conjugated mAb to CD45R/B220 (RA3-6B2), PerCP-Cy5.5-conjugated mAb to IgM (R6-60.2), and FITC-conjugated mAb to IgD (11-26c.2a), PE-Cy7 mAB to L-selectin (Ly-22). After addition of the antibody solution, the cells were incubated for 20 minutes on ice protected from light. 1mL of staining buffer was added to each tube and tubes were spun at 1000rpm for 10 minutes at 5°C. The supernatant was then aspirated and 1mL of staining buffer added to wash. This step was repeated and tubes were then stored at 4°C protected from light.

The BD LSR II Flow cell cytometer at the Wisconsin Institute of Medical Research was used for sample analysis. FlowJo (Ashland, OR) was used to analyze the raw data.

Bronchoalveolar Lavage, Nasal Airway Lavage and Small Intestinal Lavage and IgA Antibody Quantitative Analysis

After washing the skin with ethanol, a midline incision was made over the ventral neck slightly superior to the thoracic inlet to allow access to the trachea. A tracheotomy was then created and an 18g catheter attached to a tuberculin syringe was inserted. 1mL of saline was injected slowly into the lungs and collected as bronchoalveolar lavage (BAL) fluid. The same tracheotomy site was used to inject 1mL of saline cephalad and fluid exiting the nose was collected as nasal airway lavage (NAL). Aliquots were frozen at -80°C. The small intestine was removed and the lumen rinsed with 10mL Hank’s Balanced Saline Solution (HBSS; Bio Whitaker, Walkersville, MD). The luminal rinse (small intestinal lavage, SIL) was centrifuged at 2000xg for 10 minutes and supernatant aliquots were frozen at -80°C.

IgA concentration from the NAL, BAL and SIL fluid was measured by sandwich enzyme-linked immunosorbent assay (ELISA), as previously described [Sano 2009]. Fluid IgA concentrations were calculated by plotting their absorbance values on the IgA standard curve, which was calculated using a 4-parameter logistic fit with SOFTmax PRO software (Molecular Device, Sunnyvale, CA).

Statistical analysis

The data are expressed as means ± standard error of the mean. Statistical significance was determined using Student’s t-test. Differences were considered to be statistically significant at p<0.05. Statistical calculations were performed with Microsoft Excel (Microsoft, Redmond, WA) or StatView (SAS, Cary, NC).

Results

EdnrBNCC-/- animals develop intestinal inflammation in the fourth week of life

The piebald lethal mouse strain, which contains a naturally-occurring EdnrB mutation, and conventional EdnrB knockout mice experience mortality near the fourth postnatal (P) week [40,41]. We have previously confirmed a similar timing of mortality in our model of NCC conditional deletion of EdnrB, with EdnrBNCC-/- experiencing 50% mortality by P26 and 90% mortality by P32 [19]. To correlate histological evidence of colonic inflammation with this time course, we examined the distal small intestine, proximal colon and mid-colon of P21-24 and P26-29 EdnrBNCC+/- and EdnrBNCC-/- animals using the previously published Murine Enterocolitis Grading System [40] (Table 1 and Fig 1). There was evidence of inflammation in both the proximal and mid-colon of the EdnrBNCC-/- animals at P26-29. However, no inflammation was seen in the EdnrBNCC-/- animals at the early time point or in the small intestine at the later time point. Finally, no inflammation was seen in the EdnrBNCC+/- animals at either time point or anatomic location.

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Table 1. Enterocolitis Score by Anatomic Location.

https://doi.org/10.1371/journal.pone.0128822.t001

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Fig 1. EdnrBNCC-/- animals develop intestinal inflammation in the fourth week of life.

Inflammation within proximal colon and mid-colon of P26-29 EdnrBNCC+/- (Het) and EdnrBNCC-/- (Null) animals was graded using the previously published Murine Enterocolitis Grading System (Cheng, et.al., 2010). (A) There was evidence of inflammation in both the (B) proximal and (C) mid-colon of the EdnrBNCC-/- animals at the later time point. Arrows indicate inflammatory cells. Scale bar = 50 μm. (*p<0.05).

https://doi.org/10.1371/journal.pone.0128822.g001

Peyer’s Patches of EdnrBNCC-/- animals are small in size but have normal architecture

PP are distinct collections of immune cells located along the anti-mesenteric surface of the bowel; they display follicular architecture similar to lymph nodes and are the primary inductive site for gut mucosal immunity [42]. Previous observations that PP are absent in RET-/- animals and are diminished in RET51/51 hypomorphic animals [29] prompted us to investigate whether the EdnrBNCC-/- animals exhibit alterations in their GI immune apparatus. We harvested small bowel from EdnrBNCC-/- and EdnrBNCC+/- at P21-24 [19]. We found that the PP of EdnrBNCC-/- animals are smaller than those of EdnrBNCC+/- animals on gross examination (Fig 2). To quantify this, cross-sectional measurements of PP height and width were taken and area calculated. We found that EdnrBNCC-/- PP have significantly smaller cross-sectional area than EdnrBNCC+/- (EdnrBNCC+/- 1.15±0.05 mm2 vs. EdnrBNCC-/- 0.49±0.04 mm2, p = 4.1x10-17). Although smaller in size, H&E staining demonstrates that the architecture of EdnrBNCC-/- PP is preserved, with distinct germinal centers, subepithelial domes and follicle-associated epithelium (Fig 2). Additionally, while the extent of B220+ and CD3+ staining is decreased in the EdnrBNCC-/- animals, suggesting fewer cells, the distribution of B220+ B-lymphocytes and CD3+ T-lymphocytes in distinct B- and T-cell zones within the PP appears unchanged between EdnrBNCC+/- and EdnrBNCC-/- animals (Fig 2). Finally, unlike the observation in RET mutant models, we did not observe a difference in the number of PP between groups (EdnrBNCC+/- 9.75±0.85 vs. EdnrBNCC-/- 7.25±1.3, p = 0.16).

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Fig 2. Peyer’s Patches of EdnrBNCC-/- animals are small in size but have normal architecture.

(A) Gross photographs of representative PP isolated from EdnrBNCC+/- and EdnrBNCC-/- animals demonstrating the size difference. Scale bar = 1000μm. (B) H&E staining of PP cross-sections from EdnrBNCC+/- and EdnrBNCC-/- animals. Architectural features are preserved in EdnrBNCC-/-. Scale bar = 400μm (applies to B,C,D). (C) IHC of PP cross-sections with CD3 labeling T cells. (D) IHC of PP cross-sections with B220 labeling B cells. The spatial distribution of B-cells and T-cells is similar between EdnrBNCC+/- and EdnrBNCC-/-.

https://doi.org/10.1371/journal.pone.0128822.g002

Peyer’s Patches of EdnrBNCC-/- animals exhibit B-cell lymphopenia

Given their small size, we next examined the cellular composition of PP in the EdnrBNCC-/- animals. We isolated PP from EdnrBNCC+/- and EdnrBNCC-/- animals and employed mechanical dispersion to isolate lymphocytes. EdnrBNCC-/- PP were hypocellular (EdnrBNCC+/- 18x104±2x104 vs. EdnrBNCC-/- 6x104± 3x104, p = 0.0196, n = 6, Fig 3), which was expected given the smaller size as compared to EdnrBNCC+/- PP. We then performed flow cytometry, using CD3+ to identify total T-lymphocytes and B220+ to identify total B-lymphocytes (Fig 3). The proportion of total T-lymphocytes was unchanged between the two groups (EdnrBNCC+/- 19.3±0.9% vs. EdnrBNCC-/- 18.9±2.1%, p = 0.88, n = 6, S1 Fig and Table 2). Additionally, we did not see any differences in the proportions of CD3+CD4+ or CD3+CD8+ T-lymphocytes between the two groups (S1 Fig and Table 2). In contrast, the proportion of total B-lymphocytes in EdnrBNCC-/- PP was significantly decreased to ~80% of the level seen in the EdnrBNCC+/- PP (EdnrBNCC+/- 66.2±1.6% vs. EdnrBNCC-/- 55.4±3.6%, p = 0.01, Fig 3), representing a 3.6-fold reduction in the number of PP B cells (EdnrBNCC+/- 119160 vs. EdnrBNCC-/- 33240, Fig 3 and Table 2).

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Fig 3. Peyer’s Patches of EdnrBNCC-/- animals exhibit B-cell lymphopenia.

(A) Total lymphocytes (per PP) are decreased in EdnrBNCC-/- vs. EdnrBNCC+/- (*p = 0.0196). (B) Representative flow cytometry gating of PP showing CD3 and B220 to identify T- and B-lymphocytes (top) and IgD and IgM to identify B220+IgM+IgDhigh (mature) B-lymphocytes (bottom). (C) The proportion of B-lymphocytes (B220+) per PP is decreased in EdnrBNCC-/- vs. EdnrBNCC+/- (*p = 0.01). (D) The number of B-lymphocytes per PP is decreased in EdnrBNCC-/- vs EdnrBNCC+/- (calculated values). (E) The proportion of B220+IgM+IgDhigh mature B-lymphocytes is decreased in EdnrBNCC-/- vs.—het PP (*p = 0.015). (F) The number of mature B-lymphocytes per PP is decreased in EdnrBNCC-/- vs EdnrBNCC+/- (calculated values).

https://doi.org/10.1371/journal.pone.0128822.g003

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Table 2. Summary results of cellularity findings in EdnrBNCC+/- and EdnrBNCC-/- Peyer’s Patches (PP), Spleen (SPL) and Peripheral Blood (PBL).

https://doi.org/10.1371/journal.pone.0128822.t002

EdnrBNCC-/- animals demonstrate a gut-specific SIgA deficiency

B-lymphocytes in the PP are activated by antigen presentation to become IgA-producing plasma cells. These activated B-lymphocytes circulate and home to the lamina propria where they produce and secrete IgA. Secretory IgA (SIgA) is the principle effector of antigen-specific immune defense along the mucosal surface[43]. EdnrBNCC-/- animals display clinical signs of enterocolitis (lethargy, ruffled coat, decreased oral intake) around P26 with a median survival of 29 days[19]. To determine if the B-lymphocytopenia observed at P21-24 is associated with impaired functional immunity, we performed nasal airway lavage, bronchoaleveolar lavage and small intestinal lavage on EdnrBNCC+/- and EdnrBNCC-/- animals at P26 and measured SIgA by ELISA. SIgA was markedly decreased in the small intestine of EdnrBNCC-/- animals compared to EdnrBNCC+/- (EdnrBNCC+/- 106.5±56.7ng/mL vs. EdnrBNCC-/- 18±9.8ng/mL, p = 0.002, n = 6, Fig 4). No differences were seen in SIgA levels in either the nasal airway lavage (EdnrBNCC+/- 7.1±4.2pg/mL vs. EdnrBNCC-/- 6.8±2pg/mL, p = 0.95, n = 8, Fig 4) or bronchoalveolar lavage (EdnrBNCC+/- 9.1±5.4pg/mL vs. EdnrBNCC-/- 18±6.6pg/mL, p = 0.31, n = 8, Fig 4). Previous investigations in humans have demonstrated increased levels of IgM in addition to alterations in IgA in the bowel during enterocolitis[44]. To evaluate this possibility in the EdnrBNCC-/- animals, we measured IgM levels in the small intestine lavage fluid. We did not detect differences in small bowel luminal IgM between EdnrBNCC+/- and EdnrBNCC-/- animals (EdnrBNCC+/- 4.6±1.4pg/mL vs. EdnrBNCC-/- 6.8±1.7pg/mL, p = 0.3, n = 8, Fig 4).

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Fig 4. EdnrBNCC-/- animals demonstrate a gut-specific deficiency of Secretory IgA (SIgA).

Secretory IgA was measured by ELISA in (A) small intestinal lavage fluid (*p = 0.002), (B) nasal airway lavage fluid, and (C) bronchoalveolar lavage fluid of EdnrBNCC+/- and EdnrBNCC-/- animals. (D) Additionally, IgM in small intestinal lavage was measured.

https://doi.org/10.1371/journal.pone.0128822.g004

Mature B-lymphocytes are reduced in EdnrBNCC-/- PP and enriched in the spleen

A specific subset (IgM+IgDhigh) of B-lymphocytes, termed mature B-lymphocytes, in the PP are responsible for the majority of murine intestinal IgA production [45]. We re-examined P21-24 PP lymphocytes by flow cytometry (Fig 3) and found that the mature B-lymphocyte population is decreased in EdnrBNCC-/- animals (EdnrBNCC+/- 51.7±1% vs. EdnrBNCC-/- 40.4±2.3%, p = 0.015, n = 6, Fig 3). This relationship held true for numbers of PP mature B-lymphocytes as well (EdnrBNCC+/- 61605 vs. EdnrBNCC-/- 13429, Fig 3).

In the mouse, mature B-lymphocytes in PP are primarily of splenic origin [45,46]. Initial observations by Cheng, et.al. indicated the presence of small spleens and splenic lymphopenia in the conventional EdnrB knockout model of HSCR [47], indicating that the immune system defects in this animal model may extend beyond the GI tract. We have extended their analysis, in our NCC-conditional deletion of EdnrB model, that the spleens in P21-24 EdnrBNCC-/- are smaller in size than those in the EdnrBNCC+/- (Fig 5). We found that the spleens of EdnrBNCC-/- weighed significantly less than those of the EdnrBNCC+/- as a proportion of the total body weight (EdnrBNCC+/- 0.67±0.05% vs. EdnrBNCC-/- 0.39±0.06%, p = 0.02, n = 10, Fig 6). We then examined splenic architecture and noted a decrease in the size of both the white and red pulp of the EdnrBNCC-/- spleen (Fig 5). We further examined architecture by immmunostaining (Fig 5) and observed a paucity of B-lymphocytes in the germinal centers of EdnrBNCC-/- spleens, and a marked decrease of B-lymphocytes within the marginal zones, suggesting potential defects in B-lymphocyte maturation [48].

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Fig 5. The spleen of EdnrBNCC-/- animals is small in size and has abnormal architecture.

(A) Gross photographs of representative spleens isolated from EdnrBNCC+/- and EdnrBNCC-/- animals demonstrating the size difference. (B) H&E staining of spleen cross-sections from EdnrBNCC+/- and EdnrBNCC-/- animals. EdnrBNCC-/- spleens demonstrate decreased red pulp (RP) and white pulp (WP). Scale bar = 600μm. (C) IHC of spleen cross-sections with B220 (green) and CD3 (blue). There are decreased B-cells in the germinal centers and a paucity of these cells within the marginal zone, located outside the ring of MOMA+ (red) staining. Scale bar = 200μm.

https://doi.org/10.1371/journal.pone.0128822.g005

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Fig 6. The spleen of EdnrBNCC-/- animals exhibits B-cell lymphopenia.

(A) Organ weights of the spleen (*p = 0.02) as a proportion of body weight, indicating that the spleens of EdnrBNCC-/- animals are small for size. (B) Total lymphocytes (per spleen) are decreased in EdnrBNCC-/- vs. EdnrBNCC+/- (*p = 0.002). (C) Representative flow cytometry gating of splenocytes showing CD3 and B220 to identify T- and B-lymphocytes (top) and IgD and IgM to identify B220+IgM+IgDhigh (mature) B-lymphocytes (bottom). (D) The proportion of B-lymphocytes (B220+) per spleen is decreased in EdnrBNCC-/- vs. EdnrBNCC+/- (*p = 0.000053). (E) The number of B-lymphocytes per spleen is decreased in EdnrBNCC-/- vs.—het spleens (calculated values). (F) B220+IgM+IgDhigh mature B-lymphocytes are increased in EdnrBNCC-/- vs.—het spleen (*p = 0.00023). (G) The number of mature B-lymphocytes per spleen is decreased in EdnrBNCC-/- vs.—het spleens (calculated values).

https://doi.org/10.1371/journal.pone.0128822.g006

Having noted alterations in splenic architecture and distribution of lymphocytes within the parenchyma of the spleen, we then determined total lymphocyte counts in the spleens (Fig 6). We observed splenic lymphopenia in the EdnrBNCC-/- animals (EdnrBNCC+/- 2.6x107±0.19x107 vs. EdnrBNCC-/- 1.2x107±0.19x107, p = 0.002), as has previously been described in the conventional EdnrB mutants [47]. In addition, because the spleen is the primary source of IgA-producing mature B-lymphocytes in the PP, we analyzed B-lymphocyte subsets (Fig 6 and Table 2). We observed a decrease in the proportion of total (B220+) B-lymphocytes in EdnrBNCC-/- (EdnrBNCC+/- 60±1.1% vs. EdnrBNCC-/- 43.4±2.8%, p = 0.000053, Fig 6) as well as in numbers of total B lymphocytes (EdnrBNCC+/- 15600000 vs. EdnrBNCC-/- 5208000, Fig 6). In contrast to our finding in EdnrBNCC-/- PP, we observed an increase in the proportion of mature B-lymphocytes in the EdnrBNCC-/- spleen (EdnrBNCC+/- 32.9±1% vs. EdnrBNCC-/- 39.1±2%, p = 0.00023, Fig 6), although the numbers were decreased (EdnrBNCC+/- 5132400 vs. EdnrBNCC-/- 2036328, Fig 6).

To determine if the both the PP and splenic B lymphopenia we observed in the EdnrBNCC-/- animals was secondary to suppression of bone marrow lymphopoiesis, we examined the pre/pro-B lymphocyte and mature B lymphocyte populations at P21. We noted no differences in either population at this time point (pre/pro B: EdnrBNCC+/- 70.5±1.3% vs. EdnrBNCC-/- 71.8±3.6%, p = 0.76; mature B: EdnrBNCC+/- 9.6±1.1% vs. EdnrBNCC-/- 10.4±2.8%, p = 0.81).

L-selectin/MAdCAM-1 Mediated Trafficking of B-lymphocytes from Peripheral Blood to PP is preserved

B-lymphocytes targeted for mucosa-associated lymphoid tissue (e.g. PP) are identified by the cell-surface integrin L-selectin [49]. L-selectin expression is acquired by B-lymphocytes in the spleen as part of the process of normal maturation [50]. Mature B-lymphocytes expressing L-selectin (L-selectinhigh) leave the spleen, circulate in the peripheral blood, and home to the PP. To determine if the proportional increase in mature B-lymphocytes in the spleen and concurrent decrease in the PP of EdnrBNCC-/- was due to a failure of trafficking of circulating B-cells from peripheral blood to the PP, we measured the B220+IgM+IgDhighL-selectinhigh population in peripheral blood. We found no differences in the L-selectinhigh mature B-lymphocyte populations between EdnrBNCC+/- and EdnrBNCC-/- animals (EdnrBNCC+/- 35±2.7% vs. EdnrBNCC-/- 38.4±4.7%, p = 0.6, n = 9, Fig 7 and Table 2).

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Fig 7. Trafficking of B-lymphocytes from Peripheral Blood to PP is preserved.

(A) The proportion of circulating mature B-lymphocytes expressing L-selectin is unchanged between EdnrBNCC+/- and-null animals. (B) Levels of PP Mucosal Addressin Cell Adhesion Molecule-1 (MAdCAM-1) are unchanged between EdnrBNCC+/- and EdnrBNCC-/- animals.

https://doi.org/10.1371/journal.pone.0128822.g007

L-selectin interacts with Mucosal Addressin Cell Adhesion Molecule-1 (MAdCAM-1) on the high endothelial venules of the PP to mediate attachment of the lymphocytes and localization to the PP [49]. To determine if there is a defect in homing of circulating mature B-lymphocytes to the PP, we measured MAdCAM-1 in PP at P21-24 by ELISA. We found similar levels of MAdCAM-1 in PP from EdnrBNCC+/- and EdnrBNCC-/- animals (EdnrBNCC+/- 0.5±0.06 ng/mg vs. EdnrBNCC-/- 0.6±0.06ng/mg, p = 0.2, n = 10, Fig 7).

Discussion

In this study we utilized the NCC conditional deletion of EdnrB model of HSCR to systematically determine GI cellular immune defects that may contribute to the development of HAEC. In addition to recapitulating the clinical HSCR phenotype of distal colonic aganglionosis, our data indicate that loss of EdnrB specifically in the neural crest cells, and not in other cell types, is sufficient for development of the HAEC phenotype. We demonstrate that EdnrBNCC-/- animals display lymphopenia of their PP, namely a decrease in B220+IgM+IgDhigh (mature) B-lymphocytes. These observations are found prior to histologic evidence of enterocolitis, suggesting a specific B-lymphocyte defect that may contribute to the development of enterocolitis. These animals also display a gut-specific reduction of SIgA, which may be secondary to the decreased mature B-lymphocytes population in the PP. We also determined that EdnrBNCC-/- demonstrate B-lymphocytopenia of the spleen, but display an increased proportion of mature B-lymphocytes and a paucity of B-lymphocytes within the marginal zones, observations suggesting possible defects in B-lymphocyte maturation and/or egress from the spleen. Finally, we noted equivalent proportion of circulating L-selectin+ Mature B lymphocytes in EdnrBNCC+/- and EdnrBNCC-/- animals, as well as equivalent levels of MAdCAM-1 in the PP, which suggests that circulating mature B-lymphocytes are capable of trafficking to the PP in these animals. Together, these data suggest that the spleen may be the primary anatomic site of B-lymphocyte defects in EdnrBNCC-/-. Accordingly, these data are the first to demonstrate a cellular immune defect that may link the splenic immune apparatus and GI mucosal immunity in the context of HSCR.

Multiple lines of investigation point to interactions between the ENS and GI mucosal immune system. Anatomically, enteric neurons innervate the intestinal mucosa, including the gut-associated lymphoid tissue [51]. Enteric ganglia are positioned along the base, corona and interfollicular regions of PP [51–55]. Other investigators have demonstrated functional alterations in immune cell function associated with changes in the ENS, likely related to the presence of neuropeptide receptors on the surface of immune cells [56–58]. It has also been proposed that invasion of enteric nerves via the PP serves as a route of infection of the central nervous system by ingested prions [53,59].

The most common genetic defects associated with HSCR are mutations of RET and EdnrB, which are both required for NCC migration and ENS formation. RET has been identified as necessary for the development of PP [29]. In an elegant series of experiments [29,60], it has been shown that PP generation involves the aggregation of CD4+CD3−IL-7Ra+c-Kit+CD11c− lymphoid tissue inducer (LTi) cells, CD4−CD3−c-Kit+IL-7Ra−CD11c+RET+ lymphoid tissue initiator (LTin) cells, and mesenchymal lymphoid tissue organizer (LTo) cells, leading to formation of PP primordia in the midgut of mice by embryonic day 16.5 (E16.5). In the current study, we did not observe differences in the numbers of PP in EdnrBNCC-/- animals, but rather specific defects in B-lymphocyte populations within the PP and the spleen, suggesting perturbations in B-lymphocyte maturation, trafficking, or function.

Another group investigating the mechanisms of HAEC has noted reduced splenic size in EdnrB-/- animals [47]. They have additionally described abnormal splenic architecture and reduced total lymphocytes in the spleen. They postulate that this results in systemic immune deficiency that may predispose to HAEC. We noted similar findings of reduced splenic mass and altered architecture in our NCC-conditional EdnrBNCC-/-, suggesting a role for NCC or EdnrB in lymphocyte development. Endothelin ligands (ET-1, ET-3) and receptors (EdnrA, EdnrB) form the endothelin axis, which participates in diverse biological processes including development, inflammation and cancer. The role of the endothelin axis in vascular biology has been well characterized [61]. However, beyond the vascular system, endothelins and their receptors are co-expressed in a wide variety of tissues and undergo coordinated changes in expression, suggesting a tightly-regulated, autocrine-paracrine mechanism of action [61,62]. There is extensive literature demonstrating modulation of lymphocyte function by endothelins [63–66]. Additionally, components of the endothelin axis are over-expressed in the serum and bowel wall of Crohn’s disease patients [67,68] and EdnrA/B antagonists can reduce inflammation in murine models of chemically-mediated colitis [69,70], underscoring a potential role for endothelins in bowel pathology. Indeed, we have previously described increased expression of EdnrB in the microenvironment of the EdnrBNCC-/- gut [37], suggesting that alterations in the endothelin axis outside of NCC may contribute to the phenotype. Further investigation into alterations of endothelin signaling outside the neural crest in our model may shed light on the HAEC phenotype.

B-lymphocytes targeted for mucosa-associated lymphoid tissue are identified by cell-surface integrins and their destination governed by chemokine/receptor interactions [71]. Mature B-cells bearing L-selectin and α4β7 integrin (L-selectinhighα4β7low) leave the spleen and home to the PP, where they interact with MAdCAM-1 on the high endothelial venules of the PP through initial attachment (L-selectin) and rolling (α4β7) [72]. This homing is mediated by the chemokine CXCL13, expressed on the PP, and the receptor CXCR5, present on B-cells. Additionally, ET-1/EdnrB signaling mediates homing of T-cells to tumors by regulation of ICAM expression [73]. Therefore, while we did not observe differences in the circulating L-selectin+ B-lymphocyte population or PP MAdCAM-1 expression, it is possible that impaired chemokine or adhesion molecule signaling reduces trafficking of B-lymphocytes from the spleen to PP.

A mucus gel layer composed of several glycoproteins and secretory IgA (SIgA) lines the luminal border of the colon and provides a defensive barrier against pathogens and foreign particles. Multiple investigators have demonstrated alterations in subsets of mucins, a major component of this layer [15,74]. Additionally, the rate of mucin turnover in the bowel is decreased in HSCR patients [74]. Interestingly, both of these observations extend to the ganglionated as well as aganglionic regions of the bowel. Another group demonstrated an increase in IgA containing plasma cells along the length of resected aganglionic bowel from five patients with HAEC as compared to seven patients without HAEC [44]. They also demonstrated that luminal IgA (or SIgA) was reduced in the same patients, suggesting either a decrease in production or impaired transport to the lumen. We report here a similar observation of decreased luminal SIgA in the EdnrBNCC-/- animals, the first demonstration of this clinical correlate in a mouse model of HSCR/HAEC. This alteration in SIgA is accompanied by decreased PP mature B-lymphocytes, which serve as the primary source of murine SIgA. This suggests that the decreased number of B-lymphocytes may result in decreased SIgA production. However, in the current study we did not measure mucosa-associated IgA or lamina propria IgA+ plasma cells, which may be preserved and would indicate a defect in secretion, rather than production. Alternatively, our finding may be a reflection of the timing of our experiments, and that SIgA is being produced and secreted appropriately, but is rapidly bound to luminal antigens. Further functional experiments of EdnrBNCC-/- B-lymphocytes are warranted to distinguish these possibilities. Finally, we noted no differences in luminal IgM between EdnrBNCC+/- and EdnrBNCC-/- animals. An elevated level of IgM, produced primarily by lamina propria-resident B-lymphocytes, would have been unexpected because LP-resident B-lymphocytes do not typically make non-IgA isotypes until post-natal week 6 [46,75].

A notable limitation of our study is the presence of concomitant bowel obstruction secondary to distal colonic aganglionosis. The presence of the distal bowel obstruction may lead to stasis of intestinal contents, alterations in the microbiome, histologic changes, and sepsis. Certainly, previous investigations have demonstrated similar histological features in HAEC-affected bowel and obstructed bowel [14,15]. Additionally, similar changes in splenic lymphocyte populations can be found in response to sepsis/stress [76]. To dissect out the contribution of obstruction and stress to the immune phenotype of conventional EdnrB knockout animals, Frykman, et.al. have recently published a study in which they performed bone marrow transplants from EdnrB-/- animals to Rag2-/- recipients, as well as inducing bowel obstruction in WT animals [12]. In this study, they elegantly demonstrate that the stress from obstruction and the consequent elaboration of cortisone result in reductions in immune populations similar to those observed in our study and in their prior work. However, when their study is put in the context of their prior work, in which ~40% of EdnrB-/- animals develop HAEC after surgical relief of obstruction [9], one can conclude that relieving the bowel obstruction is not sufficient to prevent the development of HAEC. This result suggests that other factors contribute to the etiology of HAEC in the EdnrB-/- model. Indeed, in their recent study, Frykman, et.al. noted small splenic size in the EdnrB-/- bone marrow transplant recipients, concluding that EdnrB may play a role in lymphocyte trafficking between the bone marrow, thymus and spleen. Ultimately, our laboratory findings and those of other groups are in need of contemporary human tissue correlates in order to understand their true significance.

The increasingly challenged dogma in HSCR is that the abnormal bowel is limited to the aganglionic segment. Our data build upon the growing body of literature that suggests that intestinal defects in HSCR are not restricted to the aganglionic colon and extend proximally, even into the ganglionated small intestine. These abnormalities likely include subtle differences in extent of innervation and neuronal phenotypes, which may explain motility disturbances, as well as alterations in the microbiome composition and mucosal immune apparatus, which together may predispose to HAEC. Dissecting the mechanisms by which endothelin signaling participates in mucosal immune development will further our understanding of how the functions of the ENS and immune system are integrated and may provide insight into the development of HAEC.

Supporting Information

S1 Fig. T-lymphocyte populations in EdnrBNCC-/- PP.

(A) The proportion of T-lymphocytes (CD3+) per PP is unchanged between EdnrBNCC-/- vs. EdnrBNCC+/-. (B) The proportion of CD3+CD4+ and (C) CD3+CD8+ T-lymphocytes is unchanged between EdnrBNCC-/- vs.—het PP. (D) The number of T-lymphocytes per PP is decreased in EdnrBNCC-/- vs.—het PP (calculated values). (E) The number of CD3+CD4+ and (F) CD3+CD8+ T-lymphocytes is decreased in EdnrBNCC-/- vs.—het PP (calculated values).

https://doi.org/10.1371/journal.pone.0128822.s001

(TIF)

Author Contributions

Conceived and designed the experiments: AG. Performed the experiments: AG AJBA CSE JFP AFH. Analyzed the data: AG AJBA JFP MLE KAK. Contributed reagents/materials/analysis tools: AG MLE KAK. Wrote the paper: AG AJBA MLE. Critical revision of the manuscript: AG AJBA MLE KAK.

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