Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Avian Resistance to Campylobacter jejuni Colonization Is Associated with an Intestinal Immunogene Expression Signature Identified by mRNA Sequencing

  • Sarah Connell ,

    Affiliation Smurfit Institute of Genetics, University of Dublin, Trinity College, Dublin, Ireland

  • Kieran G. Meade,

    Affiliation Teagasc, Animal & Grassland Research and Innovation Centre, Co Meath, Ireland

  • Brenda Allan,

    Affiliation Vaccine and Infectious Disease Organization, University of Saskatchewan, Saskatoon, Canada

  • Andrew T. Lloyd,

    Affiliation School of Biochemistry and Immunology, University of Dublin, Trinity College, Dublin, Ireland

  • Elaine Kenny,

    Affiliation Trinity Genome Sequencing Laboratory, Institute of Molecular Medicine and Dept. of Psychiatry, University of Dublin, Trinity College, Dublin, Ireland

  • Paul Cormican,

    Affiliation Trinity Genome Sequencing Laboratory, Institute of Molecular Medicine and Dept. of Psychiatry, University of Dublin, Trinity College, Dublin, Ireland

  • Derek W. Morris,

    Affiliation Trinity Genome Sequencing Laboratory, Institute of Molecular Medicine and Dept. of Psychiatry, University of Dublin, Trinity College, Dublin, Ireland

  • Daniel G. Bradley,

    Affiliation Smurfit Institute of Genetics, University of Dublin, Trinity College, Dublin, Ireland

  • Cliona O'Farrelly

    Affiliation School of Biochemistry and Immunology, University of Dublin, Trinity College, Dublin, Ireland

Avian Resistance to Campylobacter jejuni Colonization Is Associated with an Intestinal Immunogene Expression Signature Identified by mRNA Sequencing

  • Sarah Connell, 
  • Kieran G. Meade, 
  • Brenda Allan, 
  • Andrew T. Lloyd, 
  • Elaine Kenny, 
  • Paul Cormican, 
  • Derek W. Morris, 
  • Daniel G. Bradley, 
  • Cliona O'Farrelly


Campylobacter jejuni is the most common cause of human bacterial gastroenteritis and is associated with several post-infectious manifestations, including onset of the autoimmune neuropathy Guillain-Barré syndrome, causing significant morbidity and mortality. Poorly-cooked chicken meat is the most frequent source of infection as C. jejuni colonizes the avian intestine in a commensal relationship. However, not all chickens are equally colonized and resistance seems to be genetically determined. We hypothesize that differences in immune response may contribute to variation in colonization levels between susceptible and resistant birds. Using high-throughput sequencing in an avian infection model, we investigate gene expression associated with resistance or susceptibility to colonization of the gastrointestinal tract with C. jejuni and find that gut related immune mechanisms are critical for regulating colonization. Amongst a single population of 300 4-week old chickens, there was clear segregation in levels of C. jejuni colonization 48 hours post-exposure. RNAseq analysis of caecal tissue from 14 C. jejuni-susceptible and 14 C. jejuni-resistant birds generated over 363 million short mRNA sequences which were investigated to identify 219 differentially expressed genes. Significantly higher expression of genes involved in the innate immune response, cytokine signaling, B cell and T cell activation and immunoglobulin production, as well as the renin-angiotensin system was observed in resistant birds, suggesting an early active immune response to C. jejuni. Lower expression of these genes in colonized birds suggests suppression or inhibition of a clearing immune response thus facilitating commensal colonization and generating vectors for zoonotic transmission. This study describes biological processes regulating C. jejuni colonization of the avian intestine and gives insight into the differential immune mechanisms incited in response to commensal bacteria in general within vertebrate populations. The results reported here illustrate how an exaggerated immune response may be elicited in a subset of the population, which alters host-microbe interactions and inhibits the commensal state, therefore having wider relevance with regard to inflammatory and autoimmune disease.


The healthy vertebrate intestine is densely colonized with a wide range of non-pathogenic microorganisms which include members of all three domains of life – the eukarya, archaea and bacteria. Co-evolution of host and intestinal microbial species over millions of years has promoted beneficial coexistence and interdependency. Local immune homeostasis in the intestine is critical for both host health and commensal survival and at the same time is required to provide effective defense against harmful pathogens. The gastrointestinal immune system is consequently highly specialized and composed of cellular and molecular components with complex functional and regulatory features [1], [2]. Association of the gut microbiota with intestinal autoimmune disease [3][5] is therefore not surprising, however recent studies have also implicated the gut commensal microbiota in development of the extraintestinal autoimmune diseases arthritis [6], [7], type I diabetes mellitus [8], [9] and the mouse model of multiple sclerosis [10], [11].

In humans, C. jejuni infection elicits an inflammatory response [12][17] which regularly causes pathological symptoms. The majority of C. jejuni cases are mild, self-limiting and pathology is restricted exclusively to the intestine but the course of infection is not always predictable and it can occasionally spread to other tissues especially in the elderly and immunocompromised, leading to significant morbidity and mortality [18][20]. Campylobacteriosis has also been associated with post-infectious sequelae such as Guillain-Barré syndrome [21], [22], its rare variant Miller Fisher Syndrome [23] and reactive arthritis [24].

In contrast to infection in humans, C. jejuni does not induce any pathology in chickens and inhabits the lower intestine in a commensal relationship. The principal site of chicken colonization is within the mucus overlying crypts of the caeca, large intestine and cloaca [25]. Histopathological studies reveal no evidence of necrosis and no significant change in crypt architecture [25][27]. Although the bacteria are not observed attached to chicken intestinal epithelial cells in vivo [25], several C. jejuni adhesins have been identified and epithelial cell attachment is believed to be required for successful colonization. Invasion of primary chicken intestinal epithelial cells has been described [28], [29], but C. jejuni survives intracellularly for only a short time and subsequently the bacteria evade the cells. Replication is not thought to occur here but most likely happens in chicken intestinal mucus, where it has been demonstrated in vitro [29], [30]. Interestingly, due to the contrasting commensal and pathogenic infections which develop in chicken and human, chicken mucin limits attachment and invasion of human primary and cultured intestinal epithelial cells, while in contrast human mucus enhances internalization [28], [31]. Adherence and invasion potential of different C. jejuni strains with human Caco-2 cells correlates with colonization ability in the chicken intestine [32], whereas chicken intestinal caecal cell invasion correlates with systemic rather than intestinal colonization level [29]. Even though C. jejuni colonizes the avian intestine in an apparently commensal relationship, systemic colonization does occur, with several studies detecting the organism extra-intestinally soon after both intra-cloacal and oral infection in the bursa of Fabricius, spleen and liver/gallbladder [29], [33][35]. It has also been found in the thymus, reproductive tract and circulating blood of commercial birds [36][38]. Although no pathology is associated with chicken colonization, an intestinal immune response to infection has been illustrated with increased cytokine expression [14], [39][42] and toll-like receptor (TLR) activation [43]. Our group has previously carried out global gene expression analysis of the immune response to C. jejuni 20 hours post-infection and demonstrated activation of several pathways, including evidence of T cell involvement [44]. Differential caecal expression 7 days after infection of 1-day old chicks has also been investigated both within and between two broiler lines which differ in their susceptibility to colonization [45], [46] and significant induction of the MAPK pathway, GTPase-mediated signal transduction and several immune genes, including some indicative of T cell and B cell activity, was found. An increase in circulating macrophages can be observed in peripheral blood 6 hours post-challenge [33]. Heterophil influx into caecal tissues just 1 day post-infection has also been reported [40], although some studies report a lack of heterophil infiltration [29], [33]. These conflicting findings are probably due to differences between chicken lines and age of infection. A systemic immune response to C. jejuni involving lymphocyte activation and immunoglobulin production, has been demonstrated in the spleen [47]. Thus an early active immune response seems to be required for colonization and its regulation critical to preventing pathology. Colonization levels within the gut vary substantially between individual chickens and several studies have illustrated that this variation in colonization susceptibility is heritable [48][50]. Resistance to caecal colonization was previously shown to be dependent on host cell lineage in three crossbred stocks of commercial chickens [48]. Consistent differential colonization between inbred chicken lines was observed as soon as 24 hours after oral challenge with C. jejuni, with results of backcrossing experiments indicating the colonization resistance observed was inherited as an autosomal dominant trait [49]. A paternal genetic effect associated with resistance to colonization has also been reported in a population of commercial broilers [50].

Here, using Illumina high-throughput short-read sequencing of caecal transcriptomes we identify differential expression patterns between mRNA isolated from colonization-resistant and colonization-susceptible birds from a single population of C. jejuni-infected chickens. We observe differential expression of genes from several key immune pathways indicating that these immunological mechanisms are fundamental in regulating C. jejuni colonization. Significantly increased expression of a range of cytokines and immune effector molecules, T cell and B cell activation and immunoglobulin production are observed. This controlled immune response is accompanied by activation of components of the renin-angiotensin system and appears to confer colonization resistance to a subset of the birds analyzed.

Results and Discussion

Infection model separates colonization-resistant and colonization-susceptible birds

Three groups of 15 chickens were initially inoculated with 3.5×10 CFU, 3.5×10 CFU and 3.5×10 CFU C. jejuni and their caecal load determined 48 hours after inoculation. No C. jejuni growth was detected on plates of caecal content from birds given the lowest dosage of 3.5×10 CFU. Growth levels on the plates from medium-dosage birds were highly variable, with 7/15 plates having a very high number of CFU (6×10 CFU/g) and no growth observed on the remaining 8 plates. All plates from the high-dosage group were colonized with levels varying from 2×10– 4×10 CFU/g. It was therefore determined that the dosage level resulting in optimal differential colonization in the flock was the medium dose of 3.5×10 CFU (Figure 1A). After inoculation of the remaining 255 chicks with 3.5×10 CFU C. jejuni, differential colonization was again observed with 38 chicks having no plate colonization and the remaining 217 chicks having colonization levels ranging from 400 CFU/g to 2.5×10 CFU/g (Figure 1B).

Figure 1. Infection model optimization and distribution of colonization levels.

(A) To determine the optimum dose where differential colonization is observed, three groups of fifteen birds were initially inoculated with low (i, 3.5 ×10), medium (ii, 3.5×10) and high (iii, 3.5×10) doses of C. jejuni, and the colonization status of their caeca estimated after 48 hours. No colonization was detected in any bird after infection with 3.5×10 CFU. All birds were colonized after high dosage. Maximum differentiation is achieved after inoculation with the medium dose of 3.5×10 CFU C. jejuni. (B) 255 birds were challenged with 3.5×10 C. jejuni and their caecal colonization status determined after 48 hours. No C. jejuni colonization could be detected in 38 birds. Colonization levels of the remaining birds varied from 2×10– 4 ×10 CFU/g with the majority of this group having very high caecal C. jejuni levels (10CFU/g C. jejuni).

Sequence alignment and transcript level estimation

14 nil-colonized and the 14 highest-colonized birds were selected for mRNA sequencing. Two RNAseq libraries were prepared from the first sample, a nil-colonized bird, and each library was sequenced using one lane of an Illumina Genome Analyzer generating an average of 8 million reads per library. Little background noise was observed between the two sequenced lanes and due to the very high correlation and high number of reads obtained, it was determined that one lane was sufficient to sequence each sample for our analysis. The remaining 27 samples were subsequently sequenced allowing one lane per sample. After filtering for low quality reads and primer contamination, 363.75 million 36 bp reads were successfully sequenced and used in the analysis. A high proportion of reads (76.0%) mapped back to the chicken genome and exon-exon boundaries. As expected due to low repeat density within the chicken genome [51], relatively few reads (only 5.6%) mapped to more than one genome region. 27.84% of reads which mapped successfully to the genome did not map to known NCBI gene models (Figure 2). A large dataset of expression level estimates is presented in this study which may facilitate future studies of coexpression dynamics and also substantially facilitate updated annotation of the chicken genome.

Figure 2. RNAseq read mapping percentage breakdown.

175.31 million (48.2%) of the reads generated from mRNA sequencing could be mapped uniquely to known gene models and therefore could be used in estimation of gene expression levels. 101.28 million reads (27.8%) were mapped successfully to the genome but could not be mapped to NCBI gene models (unknown transcripts, 3.65 Gbp) indicating a necessity for more comprehensive annotation of the chicken transcriptome. Relatively few repeat reads (20.49 million reads, 5.6%) were observed consistent with the low repeat density of the chicken genome [51].

Analysis of gene expression reveals substantial transcriptome differences between susceptible and resistant birds

The R package DESeq [52] was used to test for differential expression implementing a negative binomial model of the count data. 41 genes exhibited significant differential expression after adjustment for multiple testing (Benjamini & Hochberg p-value 0.01). Functional analysis of these genes did not uncover significant enrichment of any gene ontology (GO) terms or KEGG pathways after adjustment for multiple testing. In order to identify more subtle patterns of differential expression, a relaxed significance threshold of unadjusted p-value 0.01 was implemented and a total of 221 genes exhibited differential expression between high-colonized and nil-colonized birds at this threshold (Figure 3 and Table S1). Two of these genes (LOC776447 and LOC431338) displayed unusually high residual variance quotients compared to genes of similar expression levels. Their measures of significance were therefore considered unreliable and they were excluded from subsequent analysis. The majority (175/219, 80%) of differentially expressed genes exhibited higher expression in nil-colonized relative to high-colonized birds.

Figure 3. Detection of differentially expressed genes between high-colonized and nil-colonized birds.

Log2 fold change is plotted versus mean count numbers reflecting expression level. The R package DESeq was used to compare expression levels between the two groups of high-colonized and nil-colonized chickens and to identify genes displaying significant differential expression using a negative binomial model of the count data. 221 genes exhibiting significant differential expression with p-value 0.01 are highlighted red.

Analysis of abundance of differentially expressed genes within biological pathways using Goseq [53] did not reveal any bias introduced by differing expression levels (Figure 4), which is in agreement with the even distribution of mean count numbers among significant genes depicted in Figure 3. Functional analysis of these genes using Goseq showed a significant overrepresentation of genes involved in several KEGG pathways and gene ontology (GO) terms (FDR  = 0.05). Differentially expressed genes were also divided into two lists of genes with increased or decreased expression in nil-colonized birds relative to high-colonized birds and analyzed separately. The set of genes with increased expression was also significantly enriched for several GO terms and KEGG pathways but no significant results were obtained with the set of genes with lower expression. Significant results from this analysis are summarized in Table 1. Several immune processes were among the GO categories significantly enriched and indicated an increase in membrane composition and signaling activity in nil-colonized birds, particularly in B cells and T cells. KEGG pathway analysis also revealed differential expression of cytokines, cell adhesion molecules (CAMs) and genes within the renin-angiotensin system (RAS). Although not detected through biological pathway analysis, there was strongly increased expression of immunoglobulin genes in nil-colonized birds (Table 2).

Figure 4. Differential expression as a function of read count.

The proportion of genes differentially expressed is plotted against the total number of reads for each gene. This plot investigates whether differential expression is more likely to be detected in genes with a higher number of read counts. The green line is the probability weighting function fitted by Goseq. Flat  =  no bias present and no correction. This illustrates that the method to detect differential expression was robust against bias introduced by differing count numbers.

Table 1. GO Terms and KEGG pathways significantly enriched in differentially expressed genes.

Table 2. Immunoglobulins and non-categorized immune genes exhibiting differential expression between resistant and susceptible birds.

Another notable aspect of the increased immune response observed in nil-colonized birds was significantly greater expression of innate immune genes encoding antibacterial molecules such as lysozyme (LYZ) which degrades bacterial cell walls, NADPH oxidase organizer 1 (NOXO1) which regulates respiratory burst and toll-like receptor 1LA (TLR1LA) (Table 2). However, the proinflammatory chemokine CXCLi2 (previously IL8) displays significantly lower expression in nil-colonized relative to high-colonized birds. Numerous studies have demonstrated CXCLi2/IL8 induction in response to C. jejuni in both human [12], [13], [15], [16], [42], [54][57] and chicken [14], [39][41]. We believe the lower expression of CXCLi2 in nil-colonized birds here is due to clearance of the bacteria through the different innate immune responses described and a consequently lower inflammatory response to C. jejuni exposure. Myxovirus (influenza virus) resistance 1 (MX1), which limits replication of influenza and other viruses dependent on allele-specific expression [58][61] also displays significantly lower expression in resistant birds. MX1 is an interferon-stimulated gene (ISG) and its expression is an indicator of IFN-a/b activity. Type I IFN responses are typically associated with viral infections, but several recent reports demonstrate their induction in reponse to bacterial infection, with the effect of either facilitating or inhibiting infection [62][66]. We believe the significantly higher expression of this gene along with higher expression of Interferon-induced protein with TPRs (IFIT5) and lower expression of Interferon Regulatory Factor 4 (IRF4) in colonized birds suggests a type I IFN response in these birds which must cope with intracellular invasion. Increased expression of IFN-b and MX1 was also observed in colonized birds in a study of caecal expression 7 days after infection of a population of 1-day old chicks [46] and IFN-b secretion has been described in human dendritic cells in response to C. jejuni [67].

Immunoglobulin production

Many genes involved in production of immunoglobulin, which limits penetration of the epithelial cell layer by commensal bacteria, were found to have increased expression in nil-colonized birds (Table 2). The main immunoglobulin lambda chain gene (IGLL1) and a similar lambda chain gene (LOC769305) are significantly increased 2.1-fold and 3.7-fold respectively, as are all four upstream immunoglobulin V-type pseudogenes which are annotated on the reference genome, their fold-changes ranging from 3.3-fold to 3.8-fold. Several genes sharing homology with heavy chain variable regions are also significantly increased. In addition, the gene encoding IgJ linker protein which is required for IgA and IgM polymerization is increased 2.8-fold. The genes encoding the immunoglobulin heavy chains are not annotated in the chicken genome. In order to estimate their expression levels, alignment was conducted to the mRNA sequences of the heavy chains of IgM (X0613.1), IgA (S40610.1) and IgY (X07174.1). Expression of IgM, IgA and IgY heavy chains was significantly higher (1.9-fold, 2.0-fold and 3.0-fold respectively) in resistant birds (Table 2 and Table S1). Together, these results indicate that there is increased production of dimeric secretory IgA, IgM and IgY in the group of nil-colonized birds which is associated with resistance to colonization.

B cells in the gastrointestinal mucosa differentiate into plasma cells which secrete large amounts of immunoglobulin to both protect against infiltration of pathogenic bacteria and to control rapidly replicating commensal colonization. T cell-dependent B cell activation and high-affinity immunoglobulin production typically takes 3–5 days, which may be too slow to effectively protect the intestine from constant immune challenge. Extrafollicular B1 cells from the peritoneal cavity and intestinal lamina propria which secrete polyreactive low-affinity immunoglobulin can respond more rapidly with T cell-independent production of IgM and class-switched IgA and IgG [68][71]. Although the presence of B1 cells in the chicken is not certain, all avian B cells express CD5, similar to B1 cells, and it has been proposed that avian B cells have some functional and developmental similarity to mammalian B1 cells [72], [73]. Production of specific immunoglobulin after C. jejuni colonization of the chicken caecum has previously been shown many weeks post-infection [74], [75] but the results reported here suggest that a more rapid T cell-independent pathway of immunoglobulin production may be induced in response to infection. We believe the increased expression of IgM, IgA and IgG observed is due to increased migration, proliferation and activity of B cells in response to infection in a manner similar to that seen in mammalian B1 cells. Although it is possible this differential expression may represent a dampening down of B cell activity in colonized birds corresponding to induction of the commensal state, we believe this is very unlikely as the intestine responds to commensal colonization with increased immunoglobulin production [68], [76].

The increased immunoglobulin production observed in nil-colonized birds here affirms that an immune response has been activated in these birds which ultimately confers resistance to C. jejuni colonization. Nil-colonized birds will therefore be referred to as resistant from this point in our discussion.

Lymphocyte differentiation and activation

In accordance with the increase in immunoglobulin production observed in resistant birds, genes involved in B cell receptor (BCR) signaling also displayed significantly increased expression. BCR-mediated signaling is crucial for multiple stages of B cell development, B cell selection and activation in response to antigen and initiation of immunoglobulin diversification through somatic hypermutation [77], [78]. Several genes critical for B cell development and activation displayed increased expression in resistant birds e.g. PAX5, IRF4, AID, CD45, CD79B, DOCK8, POU2AF1, VPREB3 and the two avian CD72 paralogues (Table 3). This development and activation of B cells is characteristic of the immune response to bacteria, including commensal bacteria. Additionally, the expression of all three CXCL13 genes and the receptor CXCR5, whose products interact to control the migration of B cells are all significantly increased in resistant birds also indicating recruitment of B cells in response to the bacterium.

Table 3. Genes involved in lymphocyte development and function exhibiting significant difference in expression between resistant and susceptible birds.

We observe substantial evidence for T cell proliferation and activation in resistant birds including expression of CD4, CTLA4, CD3D, CD3E and T cell receptor alpha genes (Table 3), which are consistent with previous findings of possible T cell activation using microarrays and RT-PCR [44], [45]. Typically, the immune response to commensal bacteria within the mucosa involves T cell-independent production of immunoglobulin in extrafollicular B cells in order to limit penetration of the bacteria [79]. Although T cell-dependent IgA production has also been described [80], these mechanisms are unlikely to be involved two days post-exposure. Due to the significant differential expression of a T cell receptor alpha gene observed, this T cell response is likely to reflect greater activity of T cells. However, a T cell receptor gamma gene did also exhibit greater expression in resistant birds which almost reached significance (LOC776306, 1.65-fold, p-value  = 0.032) so involvement can not be completely excluded. Similarly, although only the CD4 gene displayed significant differential expression, the CD8A and CD8B genes demonstrated increased expression at levels almost reaching significance (Table S1). The T cell response observed may reflect greater activity of regulatory or helper T cells, both of which play a crucial role in intestinal homeostasis. Notably, the IL17 receptor E-like gene is increased over 3-fold, perhaps indicating increased response potential to T17 cells.

Several important indicators of lymphocyte activity common to both B cells and T cells, such as TNFRSF8, CCR7, IL21R and CD38 also display significantly greater expression in resistant birds (Table 3). In addition, significant evidence for positive regulation of IL2 biosynthesis is seen. IL2 is fundamental for regulatory T cell development, cytotoxic T cell differentiation, development of immunological memory, discrimination between self and non-self and can promote B cell proliferation and production of immunoglobulin [81], [82]. Its production is consistent with the other aspects of an increased immune response seen in resistant birds.

Substantial differences in expression of genes encoding cell membrane components and cell adhesion molecules are seen between resistant and susceptible birds. These differences are most probably due to the change in cellular composition of the tissue and a greater density of lymphocytes, although this may also be reflective of greater cell-cell contact and creation of a stronger membrane barrier against bacterial infiltration.

Renin-angiotensin system activation

Increased expression of genes involved in the renin-angiotensin system is seen in resistant relative to susceptible birds. This pathway principally regulates blood pressure and renal function. However, numerous studies have highlighted involvement of members of the renin-angiotensin system in inflammatory processes including regulation of T cell function [83], recruitment of inflammatory cells [84], production of reactive oxygen species [85], and autoimmune inflammation of the central nervous system [86], [87]. One of the central enzymes, Angiotensin-Converting Enzyme (ACE), has been shown to regulate DC maturation and TH1 cell development in response to Trypanosome infection in the mouse [88]. ACE overexpression in myelomonocytic lineage cells also confers an increased proinflammatory phenotype in mice which is hyperresponsive to challenge with models of lymphoma and melanoma [89], [90]. In addition, ACE overexpression increased the immune response to bacterial infection with Listeria monocytogenes and methicillin-resistant Staphylococcus aureus (MRSA) in vitro and in vivo [91]. Studies in the animal model of MS, experimental autoimmune encephalomyelitis (EAE), suggest ACE induces autoreactive T1 and T17 cells and suppresses regulatory T cells [86], [87] thus playing a significant role in autoimmune inflammation. Higher expression of the gene encoding this enzyme and other crucial genes within the renin-angiotensin system is observed here in resistant relative to susceptible birds (Table 4). This is in keeping with the other findings of an exaggerated immune response in resistant birds which obviates establishment of bacterial colonization.

Table 4. Genes involved in the renin-angiotensin system (RAS) exhibiting differential expression between resistant and susceptible birds.


In this study, we have demonstrated differential expression of genes involved in the innate immune response and lymphocyte activation associated with resistance to C. jejuni colonization in the chicken caecum. We believe the increased expression of genes involved in immunoglobulin production and B cell activity in resistant birds is due to migration, proliferation and activity of B1-like cells in response to C. jejuni. B1 cells can respond to immune challenge with a more rapid immunoglobulin response than the classical pathway involving somatic hypermutation and antigen-specific clonal expansion mediated by T cells. This B1 cell alternative activation pathway occurs in the absence of T cell help (although some T cells may play a role in its regulation) in response to T cell-independent antigens such as lipopolysaccharide, hypomethylated CpG-rich DNA, and other conserved microbial signatures which are recognized by TLRs. Strong evidence of increased T cell proliferation and activation is also seen in resistant birds, which is in agreement with previous reports of T cell activity subsequent to C. jejuni infection. This is most likely indicative of involvement of regulatory or helper T cells in the response to infection as both contribute significantly to the maintenance of intestinal homeostasis. In addition, significantly higher expression of ACE and other genes within the renin-angiotensin system is demonstrated in resistant birds. We believe this pathway is involved in amplifying the innate immune response and may be induced in response to bacterial infection, although it is possible this differential expression was present prior to infection. Further study of this pathway's involvement may be of particular relevance due to association of human C. jejuni infection with postinfectious onset of several autoimmune diseases.

Materials and Methods

Ethics Statement

This research was performed in strict accordance with the standards set by the Canadian Council on Animal Care. The protocol was approved by the Ethics Committee of the Vaccine And Infectious Disease Organization, University of Saskatchewan. Every effort was made to minimize suffering.

Infection model, microbiology and sample collection

C. jejuni strain NCTC11168v1 was grown on Meuller Hinton (MH) agar plates. The cells were resuspended in saline and viable bacterial numbers were determined on MH agar plates. 300 Barred Rock chickens were obtained from an unselected university flock, maintained by the University of Saskatchewan, Canada at one day of age. The hatchery boxes were swabbed and cultured for C. jejuni (on Karmali agar, under mixed gas, conditions at 43°C for 48 hours). The birds were reared in an animal pathogen Containment Level 2 isolation facility at the Vaccine and Infectious Disease Organization (VIDO). At 14 and 21 days of age, 20 birds were randomly chosen and cloacal swabs taken and cultured to ensure they were C. jejuni-free. On day 28 all birds were sampled by cloacal swabs and cultured. All birds were culture negative. As chickens were inoculated at 4 weeks of age, the immune system should be fully mature [92][95] and any possible anti-C. jejuni maternal antibodies not present [96]. In phase I of the infection experiment, 45 birds were separated into three groups of fifteen and challenged orally with suspensions of 3.5×10 CFU, 3.5×10 CFU and 3.5×10 CFU C. jejuni estimated by OD600 measurement. The level of C. jejuni colonization of the caecum was determined 48 hours post-inoculation. Each bird was euthanized, caecal contents removed, diluted to 0.1 g/ml and five serial 10-fold dilutions created. l of each dilution was spread on agar plates and incubated at 42°C. After 48 hours incubation the number of colony-forming units were determined for each dilution. The limit of detection for this analysis was 400 CFU/g. Subsequent to CFU quantification, phase II of the infection experiment was conducted and the remaining 255 birds were inoculated with 3.5×10 CFU C. jejuni as this was the dose where optimum colonization differentiation was achieved. Caecal content samples were again taken for microbiological culture on selectable media for quantitative analysis. Caecal tissue samples were immediately snap-frozen and stored at −80°C until mRNA isolation.

mRNA sequencing

Following quantitative analysis of colonization levels, whole caecum samples from fourteen nil-colonized and the fourteen highest-colonized birds were selected for mRNA sequencing. Total RNA was initially extracted from each sample with Trizol using the Qiagen RNeasy Lipid purification kit and diluted to g/l. All instructions in the Illumina RNA-seq protocol (Part # 1004898 Rev. A September 2008) were followed to purify mRNA and prepare samples for Illumina high-throughput sequencing. Poly-A mRNA was first isolated from total RNA using oligodT beads. The mRNA was then fragmented using divalent cations at 94°C. mRNA was converted to cDNA, blunt-ended at both ends using T4 DNA polymerase and Klenow DNA polymerase. A single A base was then added to the 3′ end to prepare for ligation to adapter sequence. cDNA templates were then size-selected by visualization and excision from agarose gel and purified. The resulting cDNA fragments were PCR-amplified and sequenced generating 40-bp reads using the Illumina Genome Analyzer.

Transcriptome alignment

Sequence image files were converted to sequence using Illumina Pipeline v1.4. Sequence reads were initially filtered for low-quality sequence and primer contamination. Each read was also trimmed by 4 bp at the 3′ end to eliminate sequences of poor quality towards the ends of the reads. To map sequences back to the transcriptome a collection of sequences representing potential splice crossing reads was created from the reference chicken genome v2.1 [51] with exon coordinates from all NCBI known gene models using Erange v3.3 [97]. The mRNA sequences encoding the heavy chains of IgM (X0613.1), IgA (S40610.1) and IgY (X07174.1) were also included. All filtered 36-bp reads were aligned with Bowtie v0.10.1 [98] to the expanded genome comprising the chicken genome, the collection of all exon-exon fasta sequences and the heavy chain mRNA sequences allowing for 3 mismatches per read and excluding reads that map to more than one position. For each individual lane, the number of counts falling on each gene model was determined with Erange using NCBI known gene models. Two lanes of the Genome Analyzer were used to sequence mRNA from the first bird analyzed – a nil-colonized chicken. The magnitude of experimental background noise between these two technical replicates was investigated by comparison to the hypergeometric distribution, as described in Marioni et al [99], and high correlation between samples was observed accompanied by a high number of reads mapping to known gene models. Therefore one lane of the Genome Analyzer was subsequently used to sequence selected polyA-mRNA from each of the 27 remaining individuals.

Identification and functional analysis of differentially expressed genes

To compare expression counts between the two groups of high-colonized and nil-colonized samples, a method for testing of differential expression where the count data are modeled with negative binomial distributions was employed in the bioconductor package DEseq v1.0.6 [52] within the R statistical environment. The cut-off used to determine significant differential expression was p-value 0.01. Fold-changes were estimated by first normalizing each read count per gene by the total number of reads per lane to obtain a RPKM measure. Functional analysis to detect enrichment of GO terms and KEGG pathways within the set of significantly differentially expressed genes was conducted using Goseq v1.0.3 [53]. To account for any selection bias of pathways arising from overrepresentation of long or overly-expressed transcripts, the dataset was corrected for read count bias.

Supporting Information

Table S1.

Analysis of differential gene expression. Genes are identified by their unique Entrez GeneID. The CGNC gene symbol and short descriptor are also provided. Average normalized gene counts for low-colonized and high-colonized birds and the fold-change between these two groups are shown. The direction of fold-change is indicated: ‘+’ reflects higher expression and ‘−’ reflects lower expression in low-colonized relative to high-colonized birds. The p-values and adjusted p-values (Benjamini & Hochberg) for each gene are shown. Although GeneID 776447 and GeneID 431338 exhibit significant differential expression, they display high residual variance and their significance estimates are therefore unreliable.



We would like to thank all staff who assisted with animal infection experiments in the Vaccine and Infectious Disease Organization at the University of Saskatchewan. Next generation sequencing was performed in the Trinity Genome Sequencing Laboratory supported by the Trinity Centre for High Performance Computing, core facilities funded by Science Foundation Ireland.

Author Contributions

Conceived and designed the experiments: SC KM BA CO DB DM EK ATL PC. Performed the experiments: SC BA EK. Analyzed the data: SC EK. Contributed reagents/materials/analysis tools: DM DB CO. Wrote the paper: SC KM CO.


  1. 1. Hill DA, Artis D (2010) Intestinal bacteria and the regulation of immune cell homeostasis. Annu Rev Immunol 28: 623–667.
  2. 2. Hooper LV, Macpherson AJ (2010) Immune adaptations that maintain homeostasis with the intestinal microbiota. Nat Rev Immunol 10: 159–169.
  3. 3. Lathrop SK, Bloom SM, Rao SM, Nutsch K, Lio CW, et al. (2011) Peripheral education of the immune system by colonic commensal microbiota. Nature 478: 250–254.
  4. 4. Kaser A, Zeissig S, Blumberg RS (2010) Inflammatory bowel disease. Annu Rev Immunol 28: 573–621.
  5. 5. Garrett WS, Lord GM, Punit S, Lugo-Villarino G, Mazmanian SK, et al. (2007) Communicable ulcerative colitis induced by T-bet deficiency in the innate immune system. Cell 131: 33–45.
  6. 6. Vaahtovuo J, Munukka E, Korkeamaki M, Luukkainen R, Toivanen P (2008) Fecal microbiota in early rheumatoid arthritis. J Rheumatol 35: 1500–1505.
  7. 7. Wu HJ, Ivanov II, Darce J, Hattori K, Shima T, et al. (2010) Gut-residing segmented filamentous bacteria drive autoimmune arthritis via T helper 17 cells. Immunity 32: 815–827.
  8. 8. Kriegel MA, Sefik E, Hill JA, Wu HJ, Benoist C, et al. (2011) Naturally transmitted segmented filamentous bacteria segregate with diabetes protection in nonobese diabetic mice. Proc Natl Acad Sci USA 108: 11548–11553.
  9. 9. Wen L, Ley RE, Volchkov PY, Stranges PB, Avanesyan L, et al. (2008) Innate immunity and intestinal microbiota in the development of Type 1 diabetes. Nature 455: 1109–1113.
  10. 10. Berer K, Mues M, Koutrolos M, Rasbi ZA, Boziki M, et al. (2011) Commensal microbiota and myelin autoantigen cooperate to trigger autoimmune demyelination. Nature.
  11. 11. Lee YK, Menezes JS, Umesaki Y, Mazmanian SK (2011) Proinflammatory T-cell responses to gut microbiota promote experimental autoimmune encephalomyelitis. Proc Natl Acad Sci USA 108 Suppl 14615–4622.
  12. 12. Hickey TE, Baqar S, Bourgeois AL, Ewing CP, Guerry P (1999) Campylobacter jejuni-stimulated secretion of interleukin-8 by INT407 cells. Infect Immun 67: 88–93.
  13. 13. Bakhiet M, Al-Salloom FS, Qareiballa A, Bindayna K, Farid I, et al. (2004) Induction of alpha and beta chemokines by intestinal epithelial cells stimulated with Campylobacter jejuni. J Infect 48: 236–244.
  14. 14. Borrmann E, Berndt A, Hanel I, Kohler H (2007) Campylobacter-induced interleukin-8 responses in human intestinal epithelial cells and primary intestinal chick cells. Vet Microbiol 124: 115–124.
  15. 15. Hu L, McDaniel JP, Kopecko DJ (2006) Signal transduction events involved in human epithelial cell invasion by Campylobacter jejuni 81–176. Microb Pathog 40: 91–100.
  16. 16. Zheng J, Meng J, Zhao S, Singh R, Song W (2008) Campylobacter-induced interleukin-8 secretion in polarized human intestinal epithelial cells requires Campylobacter-secreted cytolethal distending toxin- and Toll-like receptor-mediated activation of NF-kappaB. Infect Immun 76: 4498–4508.
  17. 17. Chen ML, Ge Z, Fox JG, Schauer DB (2006) Disruption of tight junctions and induction of proinflammatory cytokine responses in colonic epithelial cells by Campylobacter jejuni. Infect Immun 74: 6581–6589.
  18. 18. Allos BM (2001) Campylobacter jejuni Infections: update on emerging issues and trends. Clin Infect Dis 32: 1201–1206.
  19. 19. Altekruse SF, Stern NJ, Fields PI, Swerdlow DL (1999) Campylobacter jejuni–an emerging foodborne pathogen. Emerging Infect Dis 5: 28–35.
  20. 20. Wassenaar TM, Blaser MJ (1999) Pathophysiology of Campylobacter jejuni infections of humans. Microbes Infect 1: 1023–1033.
  21. 21. Tam CC, O'Brien SJ, Petersen I, Islam A, Hayward A, et al. (2007) Guillain-Barr syndrome and preceding infection with campylobacter, influenza and Epstein-Barr virus in the general practice research database. PLoS ONE 2: e344.
  22. 22. McCarthy N, Giesecke J (2001) Incidence of Guillain-Barré syndrome following infection with Campylobacter jejuni. Am J Epidemiol 153: 610–614.
  23. 23. Koga M, Gilbert M, Li J, Koike S, Takahashi M, et al. (2005) Antecedent infections in Fisher syndrome: a common pathogenesis of molecular mimicry. Neurology 64: 1605–1611.
  24. 24. Ang CW, Krogfelt K, Herbrink P, Keijser J, van Pelt W, et al. (2007) Validation of an ELISA for the diagnosis of recent Campylobacter infections in Guillain-Barré and reactive arthritis patients. Clin Microbiol Infect 13: 915–922.
  25. 25. Beery JT, Hugdahl MB, Doyle MP (1988) Colonization of gastrointestinal tracts of chicks by Campylobacter jejuni. Appl Environ Microbiol 54: 2365–2370.
  26. 26. Dhillon AS, Shivaprasad HL, Schaberg D, Wier F, Weber S, et al. (2006) Campylobacter jejuni infection in broiler chickens. Avian Dis 50: 55–58.
  27. 27. Shaughnessy RG, Meade KG, Cahalane S, Allan B, Reiman C, et al. (2009) Innate immune gene expression differentiates the early avian intestinal response between Salmonella and Campylobacter. Vet Immunol Immunopathol 132: 191–198.
  28. 28. Byrne CM, Clyne M, Bourke B (2007) Campylobacter jejuni adhere to and invade chicken intestinal epithelial cells in vitro. Microbiology (Reading, Engl) 153: 561–569.
  29. 29. Van Deun K, Pasmans F, Ducatelle R, Flahou B, Vissenberg K, et al. (2008) Colonization strategy of Campylobacter jejuni results in persistent infection of the chicken gut. Vet Microbiol 130: 285–297.
  30. 30. Hermans D, Van Deun K, Martel A, Van Immerseel F, Messens W, et al. (2011) Colonization factors of Campylobacter jejuni in the chicken gut. Vet Res 42: 82.
  31. 31. Alemka A, Whelan S, Gough R, Clyne M, Gallagher ME, et al. (2010) Purified chicken intestinal mucin attenuates Campylobacter jejuni pathogenicity in vitro. J Med Microbiol 59: 898–903.
  32. 32. Hanel I, Muller J, Muller W, Schulze F (2004) Correlation between invasion of Caco-2 eukaryotic cells and colonization ability in the chick gut in Campylobacter jejuni. Vet Microbiol 101: 75–82.
  33. 33. Meade KG, Narciandi F, Cahalane S, Reiman C, Allan B, et al. (2009) Comparative in vivo infection models yield insights on early host immune response to Campylobacter in chickens. Immunogenetics 61: 101–110.
  34. 34. Cox NA, Hofacre CL, Bailey JS, Buhr RJ, Wilson JL, et al. (2005) Presence of Campylobacter jejuni in various organs one hour, one day, and one week following oral or intracloacal inoculations of broiler chicks. Avian Dis 49: 155–158.
  35. 35. Lamb-Rosteski JM, Kalischuk LD, Inglis GD, Buret AG (2008) Epidermal growth factor inhibits Campylobacter jejuni-induced claudin-4 disruption, loss of epithelial barrier function, and Escherichia coli translocation. Infect Immun 76: 3390–3398.
  36. 36. Cox NA, Richardson LJ, Buhr RJ, Fedorka-Cray PJ, Bailey JS, et al. (2006) Natural presence of Campylobacter spp. in various internal organs of commercial broiler breeder hens. Avian Dis 50: 450–453.
  37. 37. Cox NA, Richardson LJ, Buhr RJ, Fedorka-Cray PJ (2009) Campylobacter species occurrence within internal organs and tissues of commercial caged Leghorn laying hens. Poult Sci 88: 2449–2456.
  38. 38. Richardson LJ, Cox NA, Buhr RJ, Harrison MA (2011) Isolation of Campylobacter from circulating blood of commercial broilers. Avian Dis 55: 375–378.
  39. 39. Smith CK, Kaiser P, Rothwell L, Humphrey T, Barrow PA, et al. (2005) Campylobacter jejuniinduced cytokine responses in avian cells. Infect Immun 73: 2094–2100.
  40. 40. Smith CK, Abuoun M, Cawthraw SA, Humphrey TJ, Rothwell L, et al. (2008) Campylobacter colonization of the chicken induces a proinflammatory response in mucosal tissues. FEMS Immunol Med Microbiol 54: 114–121.
  41. 41. Li YP, Ingmer H, Madsen M, Bang DD (2008) Cytokine responses in primary chicken embryo intestinal cells infected with Campylobacter jejuni strains of human and chicken origin and the expression of bacterial virulence-associated genes. BMC Microbiol 8: 107.
  42. 42. Larson CL, Shah DH, Dhillon AS, Call DR, Ahn S, et al. (2008) Campylobacter jejuni invade chicken LMH cells inefficiently and stimulate differential expression of the chicken CXCLi1 and CXCLi2 cytokines. Microbiology (Reading, Engl) 154: 3835–3847.
  43. 43. de Zoete MR, Keestra AM, Roszczenko P, van Putten JP (2010) Activation of human and chicken toll-like receptors by Campylobacter spp. Infect Immun 78: 1229–1238.
  44. 44. Shaughnessy RG, Meade KG, McGivney BA, Allan B, O'Farrelly C (2011) Global gene expression analysis of chicken caecal response to Campylobacter jejuni. Vet Immunol Immunopathol 142: 64–71.
  45. 45. Li X, Swaggerty CL, Kogut MH, Chiang HI, Wang Y, et al. (2010) Gene expression profiling of the local cecal response of genetic chicken lines that differ in their susceptibility to Campylobacter jejuni colonization. PLoS ONE 5: e11827.
  46. 46. Li XY, Swaggerty CL, Kogut MH, Chiang HI, Wang Y, et al. (2011) Caecal transcriptome analysis of colonized and non-colonized chickens within two genetic lines that differ in caecal colonization by Campylobacter jejuni. Anim Genet 42: 491–500.
  47. 47. Li X, Swaggerty CL, Kogut MH, Chiang HI, Wang Y, et al. (2012) Systemic response to Campylobacter jejuni infection by profiling gene transcription in the spleens of two genetic lines of chickens. Immunogenetics 64: 59–69.
  48. 48. Stern NJ, Meinersmann RJ, Cox NA, Bailey JS, Blankenship LC (1990) Influence of host lineage on cecal colonization by Campylobacter jejuni in chickens. Avian Dis 34: 602–606.
  49. 49. Boyd Y, Herbert EG, Marston KL, Jones MA, Barrow PA (2005) Host genes affect intestinal colonisation of newly hatched chickens by Campylobacter jejuni. Immunogenetics 57: 248–253.
  50. 50. Li X, Swaggerty CL, Kogut MH, Chiang H, Wang Y, et al. (2008) The paternal effect of Campylobacter jejuni colonization in ceca in broilers. Poult Sci 87: 1742–1747.
  51. 51. Hillier LW, Miller W, Birney E, Warren W, Hardison RC, et al. (2004) Sequence and comparative analysis of the chicken genome provide unique perspectives on vertebrate evolution. Nature 432: 695–716.
  52. 52. Anders S, Huber W (2010) Differential expression analysis for sequence count data. Genome Biol 11: R106.
  53. 53. Young MD, Wakefield MJ, Smyth GK, Oshlack A (2010) Gene ontology analysis for RNA-seq: accounting for selection bias. Genome Biol 11: R14.
  54. 54. MacCallum AJ, Harris D, Haddock G, Everest PH (2006) Campylobacter jejuni-infected human epithelial cell lines vary in their ability to secrete interleukin-8 compared to in vitro-infected primary human intestinal tissue. Microbiology (Reading, Engl) 152: 3661–3665.
  55. 55. Johanesen PA, Dwinell MB (2006) Flagellin-independent regulation of chemokine host defense in Campylobacter jejuni-infected intestinal epithelium. Infect Immun 74: 3437–3447.
  56. 56. Watson RO, Galan JE (2005) Signal transduction in Campylobacter jejuni-induced cytokine production. Cell Microbiol 7: 655–665.
  57. 57. Jones MA, Totemeyer S, Maskell DJ, Bryant CE, Barrow PA (2003) Induction of proinflammatory responses in the human monocytic cell line THP-1 by Campylobacter jejuni. Infect Immun 71: 2626–2633.
  58. 58. Ko JH, Jin HK, Asano A, Takada A, Ninomiya A, et al. (2002) Polymorphisms and the differential antiviral activity of the chicken Mx gene. Genome Res 12: 595–601.
  59. 59. Ko JH, Takada A, Mitsuhashi T, Agui T, Watanabe T (2004) Native antiviral specificity of chicken Mx protein depends on amino acid variation at position 631. Anim Genet 35: 119–122.
  60. 60. Yin CG, Zhang CS, Zhang AM, Qin HW, Wang XQ, et al. (2010) Expression analyses and antiviral properties of the Beijing-You and White Leghorn myxovirus resistance gene with different amino acids at position 631. Poult Sci 89: 2259–2264.
  61. 61. Ewald SJ, Kapczynski DR, Livant EJ, Suarez DL, Ralph J, et al. (2011) Association of Mx1 Asn631 variant alleles with reductions in morbidity, early mortality, viral shedding, and cytokine responses in chickens infected with a highly pathogenic avian influenza virus. Immunogenetics 63: 363–375.
  62. 62. Lippmann J, Muller HC, Naujoks J, Tabeling C, Shin S, et al. (2011) Dissection of a type I interferon pathway in controlling bacterial intracellular infection in mice. Cell Microbiol 13: 1668–1682.
  63. 63. Mancuso G, Midiri A, Biondo C, Beninati C, Zummo S, et al. (2007) Type I IFN signaling is crucial for host resistance against different species of pathogenic bacteria. J Immunol 178: 3126–3133.
  64. 64. Koppe U, Hogner K, Doehn JM, Muller HC, Witzenrath M, et al. (2012) Streptococcus pneumoniae stimulates a STING- and IFN regulatory factor 3-dependent type I IFN production in macrophages, which regulates RANTES production in macrophages, cocultured alveolar epithelial cells, and mouse lungs. J Immunol 188: 811–817.
  65. 65. O'Connell RM, Saha SK, Vaidya SA, Bruhn KW, Miranda GA, et al. (2004) Type I interferon production enhances susceptibility to Listeria monocytogenes infection. J Exp Med 200: 437–445.
  66. 66. Carrero JA, Calderon B, Unanue ER (2004) Type I interferon sensitizes lymphocytes to apoptosis and reduces resistance to Listeria infection. J Exp Med 200: 535–540.
  67. 67. Rathinam VA, Appledorn DM, Hoag KA, Amalfitano A, Mansfield LS (2009) Campylobacter jejuni-induced activation of dendritic cells involves cooperative signaling through Toll-like receptor 4 (TLR4)-MyD88 and TLR4-TRIF axes. Infect Immun 77: 2499–2507.
  68. 68. Cerutti A, Chen K, Chorny A (2011) Immunoglobulin responses at the mucosal interface. Annu Rev Immunol 29: 273–293.
  69. 69. Rawlings DJ, Schwartz MA, Jackson SW, Meyer-Bahlburg A (2012) Integration of B cell responses through Toll-like receptors and antigen receptors. Nat Rev Immunol 12: 282–294.
  70. 70. Pone EJ, Zan H, Zhang J, Al-Qahtani A, Xu Z, et al. (2010) Toll-like receptors and B-cell receptors synergize to induce immunoglobulin class-switch DNA recombination: relevance to microbial antibody responses. Crit Rev Immunol 30: 1–29.
  71. 71. He B, Santamaria R, Xu W, Cols M, Chen K, et al. (2010) The transmembrane activator TACI triggers immunoglobulin class switching by activating B cells through the adaptor MyD88. Nat Immunol 11: 836–845.
  72. 72. Koskinen R, Gobel TW, Tregaskes CA, Young JR, Vainio O (1998) The structure of avian CD5 implies a conserved function. J Immunol 160: 4943–4950.
  73. 73. Haghighi HR, Gong J, Gyles CL, Hayes MA, Zhou H, et al. (2006) Probiotics stimulate production of natural antibodies in chickens. Clin Vaccine Immunol 13: 975–980.
  74. 74. Cawthraw S, Ayling R, Nuijten P, Wassenaar T, Newell DG (1994) Isotype, specificity, and kinetics of systemic and mucosal antibodies to Campylobacter jejuni antigens, including flagellin, during experimental oral infections of chickens. Avian Dis 38: 341–349.
  75. 75. Myszewski MA, Stern NJ (1990) Influence of Campylobacter jejuni cecal colonization on immunoglobulin response in chickens. Avian Dis 34: 588–594.
  76. 76. Macpherson AJ, Geuking MB, McCoy KD (2012) Homeland security: IgA immunity at the frontiers of the body. Trends Immunol 33: 160–167.
  77. 77. Kurosaki T, Shinohara H, Baba Y (2010) B cell signaling and fate decision. Annu Rev Immunol 28: 21–55.
  78. 78. Harwood NE, Batista FD (2010) Early events in B cell activation. Annu Rev Immunol 28: 185–210.
  79. 79. Macpherson AJ, Gatto D, Sainsbury E, Harriman GR, Hengartner H, et al. (2000) A primitive T cell-independent mechanism of intestinal mucosal IgA responses to commensal bacteria. Science 288: 2222–2226.
  80. 80. Macpherson AJ, Harris NL (2004) Interactions between commensal intestinal bacteria and the immune system. Nat Rev Immunol 4: 478–485.
  81. 81. Ralph P, Jeong G, Welte K, Mertelsmann R, Rabin H, et al. (1984) Stimulation of immunoglobulin secretion in human B lymphocytes as a direct effect of high concentrations of IL 2. J Immunol 133: 2442–2445.
  82. 82. Mingari MC, Gerosa F, Carra G, Accolla RS, Moretta A, et al. (1984) Human interleukin-2 promotes proliferation of activated B cells via surface receptors similar to those of activated T cells. Nature 312: 641–643.
  83. 83. Hoch NE, Guzik TJ, Chen W, Deans T, Maalouf SA, et al. (February 2009) Regulation of t-cell function by endogenously produced angiotensin ii. American Journal of Physiology – Regulatory, Integrative and Comparative Physiology 296: R208–R216.
  84. 84. Ruiz-Ortega M, Bustos C, Hernandez-Presa MA, Lorenzo O, Plaza JJ, et al. (1998) Angiotensin II participates in mononuclear cell recruitment in experimental immune complex nephritis through nuclear factor-kappa B activation and monocyte chemoattractant protein-1 synthesis. J Immunol 161: 430–439.
  85. 85. Brown DI, Griendling KK (2009) Nox proteins in signal transduction. Free Radic Biol Med 47: 1239–1253.
  86. 86. Stegbauer J, Lee DH, Seubert S, Ellrichmann G, Manzel A, et al. (2009) Role of the reninangiotensin system in autoimmune inflammation of the central nervous system. Proc Natl Acad Sci USA 106: 14942–14947.
  87. 87. Platten M, Youssef S, Hur EM, Ho PP, Han MH, et al. (2009) Blocking angiotensin-converting enzyme induces potent regulatory T cells and modulates TH1- and TH17-mediated autoimmunity. Proc Natl Acad Sci USA 106: 14948–14953.
  88. 88. Scharfstein J, Monteiro AC, Schmitz V, Svensjo E (2008) Angiotensin-converting enzyme limits inflammation elicited by Trypanosoma cruzi cysteine proteases: a peripheral mechanism regulating adaptive immunity via the innate kinin pathway. Biol Chem 389: 1015–1024.
  89. 89. Shen XZ, Li P, Weiss D, Fuchs S, Xiao HD, et al. (2007) Mice with enhanced macrophage angiotensin-converting enzyme are resistant to melanoma. Am J Pathol 170: 2122–2134.
  90. 90. Shen XZ, Lukacher AE, Billet S, Williams IR, Bernstein KE (2008) Expression of angiotensinconverting enzyme changes major histocompatibility complex class I peptide presentation by modifying C termini of peptide precursors. J Biol Chem 283: 9957–9965.
  91. 91. Okwan-Duodu D, Datta V, Shen XZ, Goodridge HS, Bernstein EA, et al. (2010) Angiotensinconverting enzyme overexpression in mouse myelomonocytic cells augments resistance to Listeria and methicillin-resistant Staphylococcus aureus. J Biol Chem 285: 39051–39060.
  92. 92. Lowenthal JW, Connick TE, McWaters PG, York JJ (1994) Development of T cell immune responsiveness in the chicken. Immunol Cell Biol 72: 115–122.
  93. 93. Bar-Shira E, Sklan D, Friedman A (2003) Establishment of immune competence in the avian GALT during the immediate post-hatch period. Dev Comp Immunol 27: 147–157.
  94. 94. Bar-Shira E, Friedman A (2006) Development and adaptations of innate immunity in the gastrointestinal tract of the newly hatched chick. Dev Comp Immunol 30: 930–941.
  95. 95. Cawthraw SA, Newell DG (2010) Investigation of the presence and protective effects of maternal antibodies against Campylobacter jejuni in chickens. Avian Dis 54: 86–93.
  96. 96. Sahin O, Zhang Q, Meitzler JC, Harr BS, Morishita TY, et al. (2001) Prevalence, antigenic specificity, and bactericidal activity of poultry anti-Campylobacter maternal antibodies. Appl Environ Microbiol 67: 3951–3957.
  97. 97. Mortazavi A, Williams BA, McCue K, Schaeffer L, Wold B (2008) Mapping and quantifying mammalian transcriptomes by RNA-Seq. Nat Methods 5: 621–628.
  98. 98. Langmead B, Trapnell C, Pop M, Salzberg SL (2009) Ultrafast and memory-efficient alignment of short DNA sequences to the human genome. Genome Biol 10: R25.
  99. 99. Marioni JC, Mason CE, Mane SM, Stephens M, Gilad Y (2008) RNA-seq: an assessment of technical reproducibility and comparison with gene expression arrays. Genome Res 18: 1509–1517.