Skip to main content
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

Chicken Caecal Microbiome Modifications Induced by Campylobacter jejuni Colonization and by a Non-Antibiotic Feed Additive

  • Alexandre Thibodeau , (AT); (AL)

    Affiliations NSERC Industrial Research Chair in Meat-Safety (CRSV), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada, Swine and Avian Infectious Disease Research Centre (CRIPA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada, Groupe de recherche et d’enseignement en salubrité alimentaire (GRESA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada

  • Philippe Fravalo,

    Affiliations NSERC Industrial Research Chair in Meat-Safety (CRSV), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada, Swine and Avian Infectious Disease Research Centre (CRIPA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada, Groupe de recherche et d’enseignement en salubrité alimentaire (GRESA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada

  • Étienne Yergeau,

    Affiliation National Research Council of Canada, Montréal, Québec, Canada

  • Julie Arsenault,

    Affiliations Swine and Avian Infectious Disease Research Centre (CRIPA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada, Groupe de recherche et d’enseignement en salubrité alimentaire (GRESA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada

  • Ludovic Lahaye,

    Affiliation Jefo Nutrition Inc, Saint-Hyacinthe, Québec, Canada

  • Ann Letellier (AT); (AL)

    Affiliations NSERC Industrial Research Chair in Meat-Safety (CRSV), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada, Swine and Avian Infectious Disease Research Centre (CRIPA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada, Groupe de recherche et d’enseignement en salubrité alimentaire (GRESA), Université de Montréal, Faculty of Veterinary Medicine, Saint-Hyacinthe, Québec, Canada


Campylobacter jejuni is an important zoonotic foodborne pathogen causing acute gastroenteritis in humans. Chickens are often colonized at very high numbers by C. jejuni, up to 109 CFU per gram of caecal content, with no detrimental effects on their health. Farm control strategies are being developed to lower the C. jejuni contamination of chicken food products in an effort to reduce human campylobacteriosis incidence. It is believed that intestinal microbiome composition may affect gut colonization by such undesirable bacteria but, although the chicken microbiome is being increasingly characterized, information is lacking on the factors affecting its modulation, especially by foodborne pathogens. This study monitored the effects of C. jejuni chicken caecal colonization on the chicken microbiome in healthy chickens. It also evaluated the capacity of a feed additive to affect caecal bacterial populations and to lower C. jejuni colonization. From day-0, chickens received or not a microencapsulated feed additive and were inoculated or not with C. jejuni at 14 days of age. Fresh caecal content was harvested at 35 days of age. The caecal microbiome was characterized by real time quantitative PCR and Ion Torrent sequencing. We observed that the feed additive lowered C. jejuni caecal count by 0.7 log (p<0.05). Alpha-diversity of the caecal microbiome was not affected by C. jejuni colonization or by the feed additive. C. jejuni colonization modified the caecal beta-diversity while the feed additive did not. We observed that C. jejuni colonization was associated with an increase of Bifidobacterium and affected Clostridia and Mollicutes relative abundances. The feed additive was associated with a lower Streptococcus relative abundance. The caecal microbiome remained relatively unchanged despite high C. jejuni colonization. The feed additive was efficient in lowering C. jejuni colonization while not disturbing the caecal microbiome.


Campylobacter jejuni is the pathogen that causes campylobacteriosis, an acute gastroenteritis in humans [1]. In industrialized countries, C. jejuni is the most frequent agent associated with bacterial foodborne infections [2, 3]. A major source of infection is the consumption of undercooked chicken meat or the mishandling of raw contaminated chicken meat products [4].

It is no surprise that chicken has been identified as a major reservoir of this pathogen [5] since C. jejuni can colonize the chicken gastrointestinal tract in large numbers, frequently at levels higher than 106 CFU/g of caecal matter [6]. C. jejuni can be detected in a chicken flock at around 14 days of age and all chickens can be colonized by the end of rearing in a positive flock [7]. Experimentally, it was shown that a low dose (less than 100 CFU) of C. jejuni is sufficient for a bird’s full colonization [8]. C. jejuni mainly colonizes the chicken caecum and and is primarily presents in the mucous layer [9, 10]. This bacteria is generally recognized as having a near-commensal relationship with their chicken hosts [11], as only scarce studies have ever reported possible detrimental health effects associated with C. jejuni colonization [12]. It is still unknown how C. jejuni affects the ecology of the chicken gut.

Modern sequencing approaches [13, 14] are being used to actively characterize the chicken gut microbiome. The caecal microbiome is mainly colonized by members of the Firmicutes, Bacteriodetes, and Proteobacteria [1518]. Many of these microorganisms are thought to play an important role in chicken health, in particular, as crucial agents in the degradation of complex oligo-saccharides and the production of short-chain volatile acids [18]. The chicken intestinal microbiome matures as the chicken ages [19] and can react to numerous conditions such as feed formulations or the presence of pathogens [2023]. Despite all these advances, C. jejuni interactions within the caecal microbial community are poorly characterized.

Decreasing C. jejuni levels at the farm would be an optimal way to reduce the incidence of human campylobacteriosis acquired from chicken-associated sources [5]. Despite active research, no control method has yet been successfully and commercially implemented in the chicken industry to control this pathogen. While C. jejuni negative chicken lots can be achieved through tremendous biosecurity efforts [24], taking this route may not be feasible for the vast majority of chicken farms. One possible approach to reduce C. jejuni levels in the chicken gut is the inclusion of additives in bird feed that could lower C. jejuni caecal colonization by either direct action or by the modulation of the chicken caecal microbiome. Some essential oils and short-chain fatty acids are active in vitro against C. jejuni and have proven efficient, to varying degrees, at lowering chicken colonization [25]. The exact effect of these molecules on the modification of the chicken gut microbial ecology remains largely understudied.

The aim of this study was to assess the chicken caecal microbiome diversity changes induced by C. jejuni colonization. The study design was also used to evaluate the capacity of a microencapsulated feed additive, based on organic acids and essential oils, to influence caecal microbiome diversity and to reduce caecal C. jejuni levels.

Material and Methods

Animal model

All animal experimentations were approved by the Comité d’éthique sur l’utilisation des animaux (CEUA) of the veterinary faculty of the Université de Montréal, following guidelines from the Canadian Council on Animal Care (CCAC).

For this experiment, 4 groups were used. Chickens were inoculated or not with C. jejuni and received or not the feed additive. The two Campylobacter positive groups (group 1 and group 2) included 16 chickens each while the non-inoculated groups (group 3 and group 4) were composed of 8. The feed additive (Jefo Nutrition Inc., Saint-Hyacinthe, Canada), consisting of a microencapsulated mix of short chain organic acids and phenolic essential oils (the main ingredients being thymol and sorbic acid), was administered in feed at 2,000 ppm to group 1 and to group 3.

Day-old Ross 308 chickens, acquired from a local hatchery, were randomly assigned to one of the groups and immediately fed or not the feed additive. Chickens were raised in isolated concrete floored pens with wood shavings in the avian research center of the veterinary medicine faculty under a level two biosecurity confinement. Chickens had access to feed and water ad-libitum. Chickens were fed a standard starter diet up to 21 days of age and then received a finisher diet. Chickens were orally inoculated at 14 days of age with a mixed suspension of C. jejuni containing an equal amount of our lab strains A2008a and G2008b. These 2 strains, recovered from fresh chicken caecal content, were previously extensively characterized for their ability to colonized the chicken and compete for colonization, even in the presence of essential oils given as a feed additive [26, 27]. Each chicken received 104 CFU of each strain. This inoculum was obtained by suspending in buffered peptone water (LabM, Heywook, UK) an overnight culture of both strains grown on blood agar (Fisher Scientific, Ottawa, Canada). The inoculum concentration was validated by direct enumeration on mCCDA plates (Oxoïd, Ottawa, Canada). At 35 days of age, chickens were anesthetised by electronarcosis before being ethically killed by exsanguination. Fresh caecal content was recovered at this time and sent on ice to the laboratory for C. jejuni enumeration or immediately frozen in liquid nitrogen for further molecular analysis.

Campylobacter jejuni caecal content counts

For each chicken, 1g of caecal content was used for the enumeration of Campylobacter on mCCDA plates [28]. Caecal contents from the inoculated group were serially diluted and 100 μl of the diluted samples were plated and incubated for 48h in a microaerobic atmosphere (Oxoid) at 42°C prior to enumeration [29].

Caecal content DNA extraction

A 250 μg aliquot of the frozen caecal content was added to 500 μl of lysis buffer (Tris-HCl 500 mM pH 8, EDTA 100 mM pH 8, NaCl 100mM, SDS 1% (w/v)) and to 500 mg of 0.1mm glass beads. A MP Biomedical FastPrep instrument was used to mechanically lyse the samples, using 2 runs of 30 seconds at maximum speed. Samples were kept on ice between both runs, heated to 95°C for 10 minutes, then put back on ice. Debris and glass beads were removed by centrifugation at 10,000 g for 5 minutes. The DNA was extracted from the supernatant using a standard phenol/chloroform DNA extraction [30]. The final samples were quantified and analyzed by Nanodrop (ND 1000). Samples with ratios over 1.8 for absorbance of 260 nm/280 nm or 260 nm/230 nm were kept. DNA was stored at -20°C for further analysis.

Real time quantitative PCR of specific bacterial populations

Real time PCR was used to monitor some specific bacterial populations regularly used as indicators in classic analysis of the intestinal microbiome: total E.coli/Shigella [31], Clostridium perfringens [32], Lactobacilli [33], Enterobacteria [33], and Bifidobacterium [34]. Standard curve for all QPCR was constructed with known copy numbers of diluted PCR templates. For each QPCR reaction, 50 ng of DNA was amplified in a Roche LC96 Real Time PCR using Evagreen master mix (Montréal biotech, Montréal, Canada) in a 20 μl volume. Results were expressed as the log of target gene per 10 ng of amplified DNA.

Ion Torrent 16S rRNA gene sequencing

For a broader and detailed view of the possible microbiome modulation induced by C. jejuni, 16S rRNA gene sequencing (V2-V3 region) was performed using Ion Torrent sequencing using forward primer TACGGRAGGCAGCAG and reverse primer ATTACCGCGGCTGCTGGC [14]. For 8 chickens per group, selected according to their C. jejuni status, 20 ng of DNA was pre-amplified using a MID forward primer (0.5 μM) and a universal reverse primer (0.5 μM) in a final 50 μl reaction using Platinum PCR Supermix polymerase (Invitrogen, Burlington, Canada). The amplification was carried out for 25 cycles with a denaturation step at 95°C for 30 s, an annealing step at 55°C for 30 s, and an elongation step of 45 s at 72°C. PCR products (approximately 190 pb) were purified by gel electrophoresis using the PureLink Quick Gel Extraction Kit (Invitrogen). Purified amplicon were pooled and sequenced according to Sanschagrin and Yergeau [14].

Ion torrent data analysis

All sequencing data were analyzed [35] using Mothur v1.33 [36], based on the standard operative procedures available online, with the modifications below. When not specified, default values were used for Mothur commands.

Sequences were first trimmed using the trim.seqs command and using a qaverage score of 20, a minimum length of 100 nucleotides, and a window of 35 nucleotides. The forward primer was also kept.

For the relative abundance analysis, the sequences were then classified using a cut off of 51 percent similarity and the Greengenes database

For diversity analysis, sequences were further processed. The unique.seqs command was used to lower the computer processing load needed for analysis. Sequences were aligned against the Greengenes alignment file, using flip = true and a ksize of 6. Badly aligned sequences were removed using the screen.seqs command with the optimization set to the start of the aligned sequences and with the minimum length parameter set to 100 nucleotides. Remaining aligned sequences were filtered with the filter.seqs command. Sequences were then clustered using the pre-cluster command to correct for the effect of eventual sequencing errors diversity measurements [37]. A distance matrix was then built using the distance.seqs command with the cut-off set to 0.03. Sample coverage and diversity indexes were calculated with the summary.single command using a subsample size consisting of the lowest OTU number present in a single bird. For beta-diversity analysis, distance matrix were calculated using the distance.shared command and using the subsample = true parameter. All calculated distance matrix were visualized in a PCoA or NMDS graph. Loading and stress files were observed. The thetaYC distance matrix visualized in the NMDS plot was kept as this option was the one showing the best coverage of the total variance in the data. AMOVA and UniFrac unweighted analyses were then carried using the thetaYC phylip file. The raw sequences can be accessed via the NCBI SRA database under accession number SRA245401.

Statistical analysis

A bird was chosen for the unit of analysis. Campylobacter counts between groups were compared using a Mann-Whitney test. QPCR results, relative abundance of taxon, and diversity indexes were compared across all groups with a Kruskal-Wallis test followed by Dun’s post-hoc tests. A Mann-Whitney test was then used to compare the relative abundance of taxon found in groups relative to their Campylobacter colonization status or to their feed being supplemented or not with the feed additive. Statistical analyses were run in GraphPad v6 (Prism, LaJolla, USA). An alpha value of 0.05 was chosen as the significance level. All presented results are statistically significant unless otherwise mentioned.


Campylobacter counts in caecal content

No Campylobacter was found in the non-inoculated group (Fig 1). Campylobacter counts for the feed additive group were lower by 0.7 log in comparison to the counts of the inoculated group not supplemented with the feed additive (Fig 1).

Fig 1. Campylobacter caecal counts in chickens at 35 days of age.

No Campylobacter could be detected for the Campy- groups; each point represents the caecal content of a single chicken; horizontal bars illustrate the mean for each group; insufficient caecal matter was recovered from some chicken to allow the enumeration of C. jejuni; ** indicates p<0.01.

Real time quantitative PCR of specific bacterial populations

Standard curve efficiencies varied between 96% and 110% while all correlation coefficients (R2) were 1.0. A difference was seen between the groups for Bifidobacterium (Fig 2): detected Bifidobacterium 16S rRNA gene copies were higher by 0.4 log in the Campylobacter positive groups (p<0.001). No differences were seen for E.coli/Shigella (S1 Fig, Clostridium perfringens (S2 Fig), Lactobacilli (S3 Fig) and Enterobacteria (S4 Fig).

Fig 2. Bifidobacterium 16S copies in caecal content at 35 days of age across all chicken groups; * indicates p<0.05.

Each point represents the caecal content of a single chicken; horizontal bars illustrate the mean for each group.

16S rRNA gene sequencing

For the Campy-/Additive + group, only 6 chicken’s samples were retained for sequencing. After trimming, a total of 178 767 sequences were retained for further analysis. Prior to the diversity analysis, the average number of OTU obtained were 3 659, 3 920, 7 525 and 5 382 respectively for group 1 to 4 while the minimum numbers of sequences respectively were 898, 1 545, 3 684 and 1 518 and the maximum numbers of OTU obtained were 6 259, 6 880, 12 260 and 8 726. Analyzed alpha-diversity parameters, using a subsample of 898 OTUs which correspond to the lowers total OTU recovered from a single chicken after sequence analysis, are presented in Table 1. Neither the colonization by C. jejuni nor the use of the feed additive modified the caecal microbiome alpha-diversity.

Table 1. Comparison of alpha-diversity indexes across chicken groups and according to C. jejuni colonization or to feed additive use.

The beta-diversity was also investigated: non-metric multidimensional scaling 2 axis plots are presented in Figs 3 and 4 while analysis of molecular variance (AMOVA) and Unifrac unweighted comparisons are shown in Table 2. The colonization of chickens by C. jejuni affected the beta-diversity while no effect from the feed additive could be observed.

Fig 3. NMDS plot illustrating the chicken microbiome beta-diversity according to C. jejuni status.

Each point represents a single chicken caecal microbiome; based on a subsample of 898 OTU.

Fig 4. NMDS plot illustrating the chicken microbiome beta-diversity according to feed additive use.

Each point represents a single chicken caecal microbiome; based on a subsample of 898 OTU.

Table 2. Beta-diversity analysis across chicken groups and according to C. jejuni colonization or feed additive use.

Taxonomic analysis, based on relative abundance of the identified taxon, revealed that C. jejuni colonization induced changes in the relative abundance of detected sequences (Table 3). The main differences were observed for Mollicutes and Clostridia. No Campylobacter sequence was detected in the C. jejuni free chickens while sequences were obtained in all inoculated groups. Apart from a modulation of Streptococcus and Dehalobacteriaceae relative abundance, groups fed or not with the additive did not vary in terms of relative microbiome composition. Relative abundances of each taxonomic unit for each individual chicken sample are available in the supplemental material (S1 Table).

Table 3. Changes in the relative abundance of the caecal microbiome phylum induced by C. jejuni colonization.


In this study, we investigated the modification of the chicken caecal microbiome induced by the colonization of chickens by C. jejuni. We also tested the ability of a chicken feed additive to decrease the colonization level of this important foodborne pathogen and we monitored any associated modification of the chicken caecal microbiome. In this study’s experimental conditions, chickens were highly colonized by C. jejuni and the use of the feed additive lowered the caecal C. jejuni count by 0.7 log CFU/g.

In other studies, colonization levels of C. jejuni in broiler chickens were shown to be decreased by essentials oils or organic acids [38, 39] or to remain unaffected [40]. A synergistic effect on C. jejuni was also observed when both organic acids and botanicals were used as a feed additive [39]. It has been determined that a reduction of the C. jejuni chicken carcass contamination by 2 log would reduce the human campylobactersiosis risk by 30 [5]. Lowering the overall C.jejuni caecal load in chicken prior to slaughter is a good step toward this goal.

We observed a conservation of caecal microbiome alpha-diversity during either high colonization by C. jejuni or the use of the feed additive. Similar effects were also observed with Salmonella Enteritidis colonization in young chickens [41]. This study’s results strongly suggest that C. jejuni may become an important member of the chicken caecal microbiome without altering caecal alpha-diversity. In many other studies [19, 41], conditions tested also did not affect caecal microbiome alpha-diversity, not even necrotic enteritis [42], a severe chicken gut disorder. In another study, a severe necrotic enteritidis could be associated with changes in alpha and beta diversity [21]. Overall, based on our results and on these studies, it appears that only some drastic event that alters the number of ecological niches available to different bacterial species could modify the alpha-diversity of the chicken caecal microbiome.

In this study, beta-diversity of the chicken’s microbiome was also investigated. In our study conditions, NMDS plots highlighted differences between the birds microbiome composition, even in birds belonging to the same group. This was also reported in another study [42]. Nevertheless, the visual analysis of the NMDS graph suggested that the caecal microbiome beta-diversity was moderately affected by C. jejuni colonization and not by the additive. This was confirmed by the AMOVA and UniFrac analyses and was clearly reflected by what was observed when comparing the taxonomic rank relative abundances. The moderate but significant beta-diversity change induced by C. jejuni was quite unexpected—prior to the study we hypothesized that a high level of colonization would bring pronounced changes to the caecal microbiome ecology. In an early DGGE experiment, C. jejuni colonization was shown to affect the development and complexity of the microbial communities of the caeca over 17 days of age, in a day-old C. jejuni model [43]. More recently, another study observed in change in bacterial diversity associated with C. jejuni caecal presence in chicken without being able to clearly identify any significant changes in the microbiome composition [44].

In a recent experiment [45], Campylobacter carriage, assessed for birds originating from different farms and production types, was associated with moderate modulations of the caecal microbiome in birds of 56 days of age, sampled at slaughter houses. This study reported an increase in Streptococcus and Blautia relative abundance while a decrease was observed in the present study. The Kaakoush study also shown an association of C. jejuni presence with the relative abundance of taxon (Escherichia, Alistipes, Enterococcus, Bacteroïdes, Shigella, Gallibacterium, Lactobacillus, Corynebacterium, Ruminococcaceae, and Enterobacter), which was not observed in our study. Our study design is quite different than what was reported by Kaakoush. We measured chicken microbiome modifications solely induced by C. jejuni during a controlled experimental challenge with chickens fed mash feeds. Despite these disparities, some microbiome modifications were common in both studies–Faecalibacterium and some Clostridium increased their relative abundance when C. jejuni colonized the chicken caecum.

In this study, we confirmed the link existing between C. jejuni and Clostridium. In another study, a correlation was found between high C. perfringens levels (> 6 log) and C. jejuni colonization levels [46]. In our study conditions, this relative abundance increase of Clostridium was not due to C. perfringens levels, as demonstrated by the analysis of the C. perfringens QPCR results (S2 Fig). To explain this relationship, it was suggested that Clostridium organic acid production could be used by C. jejuni as an energy source [45]. These organic acids are also used as an energy source by chickens [47]. C. jejuni could also act as a hydrogen sink that would allow better growth of some Clostridium through increased fermentation, leading to increased organic acid production [45]. This Campylobacter-Clostridium relationship still needs to be better documented and the exact species that could be interacting needs to be examined. In our study, a Christensenellaceae (closely related to Clostridium) relative abundance increase was also induced by C.jejuni colonization. This is a relatively new family of bacteria [48] and its involvement in chicken health is unknown.

The association of C. jejuni and Faecalibacterium needs to be put into perspective. Faecalibacterium is closely related to members of Clostridium cluster IV [49]. In humans, it was shown that a decrease of Faecalibacterium prausnitzii was associated with intestinal disorders such as colitis [50]. Faecalibacterium prausnitzii is also a butyrate producer [51] and is located near the epithelial cells as it attaches to the mucous layer [49]. If this can be transposed to chickens, Faecalibacterium could be considered to share an ecological niche with Campylobacter in chickens. Its ability to produce butyrate appears to be in contradiction with its positive association with C. jejuni since butyrate was reported to be detrimental to C. jejuni [52]. It is also proposed, in humans, that Faecalibacterium prausnitzii could modulate the production of mucins by the goblet cells [53]. If this effect is also true in chickens, we hypothesize that it could be beneficial to C. jejuni as the mucous layer is believed to interfere with the organic acid anti-Campylobacter effect [7]. How Campylobacter could positively interact with Faecalibacterium and the relative importance of Faecalibacterium for chicken intestinal health remains to be determined experimentally.

In this study, a diminution of the relative abundance of Mollicutes and Anaeroplasmateles (Mollicutes class) was induced by C. jejuni colonization. In past studies, it was reported that Mollicutes were enriched in birds affected by the intestinal disease necrotic enteritidis and thus could possibly be associated with intestinal disorders for chickens [42]. The exact role of Mollicutes in the chicken microbiome is still unknown.

We observed an increase in the molecular detection of Bifidobacterium induced by C. jejuni colonization. Bifidobacterium increased levels were often associated with better gut health [54] but were also reported to hinder C. jejuni [55, 56]. It is therefore impossible to conclude if the changes observed in regards to Bifidobacterium levels were beneficial for chicken caecal health, in this study’s conditions. This observation could only be made by QPCR and not by the Ion Torrent analysis. The QPCR detected low levels of Bifidobacterium, probably too low to be picked by the Ion Torrent analysis. This could indicate that subtle changes, undetected by 16S sequencing, could still be occurring during C. jejuni colonization.

For the feed additive, an interesting decrease of Streptococcus relative abundance was also observed, which might be a good addition to its reduction of C. jejuni colonization since Streptococcus can cause diseases in chickens [57].

This study’s results suggested that the tested feed additive did not greatly imbalance the caecal microbiome. Modifications of the broilers caecal microbiome could be associated with the use of organic acids or essential oils in a previous study [58]. However, it has also been reported that essential oils were not always proven to be able to disturb the chicken caecal microbiome even when some beneficial effects on the bird’s health could be recorded [59]. It would also be interesting to verify the effect of the feed additive on the ileal microbiome as modifications of other segments of the chicken gut have not always been found to be reflected in the caecum [60].


Based on these presented results, we conclude that C. jejuni colonization induced a moderate alteration of the chicken caecal microbiome diversity. This modification did not appear to be toward undesirable bacterial populations. This is in accordance with the fact that C. jejuni rarely causes harm to the birds when colonizing the chicken caecum. Based on these study observations, it can be concluded that the chicken caecal microbiome is stable and not extensively disturbed when colonized by foodborne pathogens such as C. jejuni. We also conclude that the feed additive used was able to significantly reduce C. jejuni colonization and that it could potentially reduce Streptococcus abundance in chicken caecal contents.

Supporting Information

S1 Fig. E.coli/Shigella yccT copies in caecal content at 35 days of age across all chicken groups.


S2 Fig. Clostridium perfringens 16S copies in caecal content at 35 days of age across all chicken groups.


S3 Fig. Lactobacilli 16S copies in caecal content at 35 days of age across all chicken groups.


S4 Fig. Enterobacteria 16S copies in caecal content at 35 days of age across all chicken groups.


S1 Table. Relative abundance of each taxonomic unit found within each individual chicken sample.



We thank the following for their financial support: Ministère de l’Agriculture et des Pêches du Québec (MAPAQ), the Centre de Recherche en Infectiologie Porcine et Aviaire (CRIPA), and Natural Sciences and Engineering Research Council of Canada (NSERC grant no: 130565330; for the NSERC Industrial Research Chair in Meat Safety and other financial partners).

Author Contributions

Conceived and designed the experiments: AT PF LL AL. Performed the experiments: AT EY. Analyzed the data: AT PF EY JA. Wrote the paper: AT PF EY JA LL AL.


  1. 1. Cean A, Stef L, Simiz E, Julean C, Dumitrescu G, Vasile A, et al. Effect of human isolated probiotic bacteria on preventing Campylobacter jejuni colonization of poultry. Foodborne Pathog Dis. 2015;12(2):122–30. pmid:25585278.
  2. 2. Gras LM, Smid JH, Wagenaar JA, de Boer AG, Havelaar AH, Friesema IHM, et al. Risk Factors for Campylobacteriosis of Chicken, Ruminant, and Environmental Origin: A Combined Case-Control and Source Attribution Analysis. Plos One. 2012;7(8). ARTN e42599 WOS:000307284100139.
  3. 3. Hermans D, Pasmans F, Messens W, Martel A, Van Immerseel F, Rasschaert G, et al. Poultry as a Host for the Zoonotic Pathogen Campylobacter jejuni. Vector-Borne Zoonot. 2012;12(2):89–98. WOS:000300267700001.
  4. 4. Luber P, Brynestad S, Topsch D, Scherer K, Bartelt E. Quantification of Campylobacter species cross-contamination during handling of contaminated fresh chicken parts in kitchens. Appl Environ Microb. 2006;72(1):66–70. WOS:000234662800007.
  5. 5. Rosenquist H, Nielsen NL, Sommer HM, Norrung B, Christensen BB. Quantitative risk assessment of human campylobacteriosis associated with thermophilic Campylobacter species in chickens. Int J Food Microbiol. 2003;83(1):87–103. WOS:000182692300008. pmid:12672595
  6. 6. Hermans D, Pasmans F, Heyndrickx M, Van Immerseel F, Martel A, Deun K, et al. A tolerogenic mucosal immune response leads to persistent Campylobacter jejuni colonization in the chicken gut. Crit Rev Microbiol. 2012;38(1):17–29. WOS:000299093000002. pmid:21995731
  7. 7. Hermans D, Van Deun K, Martel A, Van Immerseel F, Messens W, Heyndrickx M, et al. Colonization factors of Campylobacter jejuni in the chicken gut. Vet Res. 2011;42. Artn 82 WOS:000293962900001.
  8. 8. Laisney MJ, Gillard MO, Salvat G. Influence of bird strain on competitive exclusion of Campylobacter jejuni in young chicks. Brit Poultry Sci. 2004;45(1):49–54. WOS:000189257000007.
  9. 9. Sylvester FA, Philpott D, Gold B, Lastovica A, Forstner JF. Adherence to lipids and intestinal mucin by a recently recognized human pathogen, Campylobacter upsaliensis. Infect Immun. 1996;64(10):4060–6. WOS:A1996VJ79400016. pmid:8926069
  10. 10. Van Deun K, Pasmans F, Ducatelle R, Flahou B, Vissenberg K, Martel A, et al. Colonization strategy of Campylobacter jejuni results in persistent infection of the chicken gut. Vet Microbiol. 2008;130(3–4):285–97. WOS:000258361500008. pmid:18187272
  11. 11. Smith CK, AbuOun M, Cawthraw SA, Humphrey TJ, Rothwell L, Kaiser P, et al. Campylobacter colonization of the chicken induces a proinflammatory response in mucosal tissues. Fems Immunol Med Mic. 2008;54(1):114–21. WOS:000259025100012.
  12. 12. Humphrey S, Chaloner G, Kemmett K, Davidson N, Williams N, Kipar A, et al. Campylobacter jejuni Is Not Merely a Commensal in Commercial Broiler Chickens and Affects Bird Welfare. Mbio. 2014;5(4). UNSP e01364–14 WOS:000341588100035.
  13. 13. Rothberg JM, Hinz W, Rearick TM, Schultz J, Mileski W, Davey M, et al. An integrated semiconductor device enabling non-optical genome sequencing. Nature. 2011;475(7356):348–52. WOS:000292911200036. pmid:21776081
  14. 14. Yergeau E, Lawrence JR, Sanschagrin S, Waiser MJ, Korber DR, Greer CW. Next-Generation Sequencing of Microbial Communities in the Athabasca River and Its Tributaries in Relation to Oil Sands Mining Activities. Appl Environ Microb. 2012;78(21):7626–37. WOS:000309678600016.
  15. 15. Qu A, Brulc JM, Wilson MK, Law BF, Theoret JR, Joens LA, et al. Comparative Metagenomics Reveals Host Specific Metavirulomes and Horizontal Gene Transfer Elements in the Chicken Cecum Microbiome. Plos One. 2008;3(8). Artn E2945 WOS:000264412600031.
  16. 16. Wei S, Morrison M, Yu Z. Bacterial census of poultry intestinal microbiome. Poultry Sci. 2013;92(3):671–83. WOS:000319314800011.
  17. 17. Oakley BB, Lillehoj HS, Kogut MH, Kim WK, Maurer JJ, Pedroso A, et al. The chicken gastrointestinal microbiome. Fems Microbiol Lett. 2014;360(2):100–12. WOS:000345457200003. pmid:25263745
  18. 18. Sergeant MJ, Constantinidou C, Cogan TA, Bedford MR, Penn CW, Pallen MJ. Extensive Microbial and Functional Diversity within the Chicken Cecal Microbiome. Plos One. 2014;9(3). ARTN e91941 WOS:000333355300046.
  19. 19. Oakley BB, Buhr RJ, Ritz CW, Kiepper BH, Berrang ME, Seal BS, et al. Successional changes in the chicken cecal microbiome during 42 days of growth are independent of organic acid feed additives. Bmc Vet Res. 2014;10. Artn 282 WOS:000347025800001.
  20. 20. Giannenas I, Papadopoulos E, Tsalie E, Triantafillou E, Henikl S, Teichmann K, et al. Assessment of dietary supplementation with probiotics on performance, intestinal morphology and microflora of chickens infected with Eimeria tenella. Vet Parasitol. 2012;188(1–2):31–40. WOS:000306617800006. pmid:22459110
  21. 21. Stanley D, Wu SB, Rodgers N, Swick RA, Moore RJ. Differential Responses of Cecal Microbiota to Fishmeal, Eimeria and Clostridium perfringens in a Necrotic Enteritis Challenge Model in Chickens. Plos One. 2014;9(8). ARTN e104739 WOS:000341303700013.
  22. 22. Singh P, Karimi A, Devendra K, Waldroup PW, Cho KK, Kwon YM. Influence of penicillin on microbial diversity of the cecal microbiota in broiler chickens. Poultry Sci. 2013;92(1):272–6. WOS:000313306700035.
  23. 23. Videnska P, Faldynova M, Juricova H, Babak V, Sisak F, Havlickova H, et al. Chicken faecal microbiota and disturbances induced by single or repeated therapy with tetracycline and streptomycin. Bmc Vet Res. 2013;9. Artn 30 WOS:000315722000001.
  24. 24. Newell DG, Elvers KT, Dopfer D, Hansson I, Jones P, James S, et al. Biosecurity-Based Interventions and Strategies To Reduce Campylobacter spp. on Poultry Farms. Appl Environ Microb. 2011;77(24):8605–14. WOS:000298157800018.
  25. 25. Hermans D, Van Deun K, Messens W, Martel A, Van Immerseel F, Haesebrouck F, et al. Campylobacter control in poultry by current intervention measures ineffective: Urgent need for intensified fundamental research. Vet Microbiol. 2011;152(3–4):219–28. WOS:000294937500002. pmid:21482043
  26. 26. Thibodeau A, Fravalo P, Taboada EN, Laurent-Lewandowski S, Guevremont E, Quessy S, et al. Extensive characterization of Campylobacter jejuni chicken isolates to uncover genes involved in the ability to compete for gut colonization. Bmc Microbiol. 2015;15. Artn 97 WOS:000354079900001.
  27. 27. Thibodeau A, Fravalo P, Garneau P, Masson L, Laurent-Lewandowski S, Quessy S, et al. Distribution of Colonization and Antimicrobial Resistance Genes in Campylobacter jejuni Isolated from Chicken. Foodborne Pathog Dis. 2013;10(4):382–91. WOS:000317353400013. pmid:23510494
  28. 28. Hutchinson DN, Bolton FJ. Improved Blood Free Selective Medium for the Isolation of Campylobacter Jejuni from Fecal Specimens. J Clin Pathol. 1984;37(8):956–7. WOS:A1984TE90600023.
  29. 29. Thibodeau A, Fravalo P, Laurent-Lewandowski S, Guevremont E, Quessy S, Letellier A. Presence and characterization of Campylobacter jejuni in organically raised chickens in Quebec. Can J Vet Res. 2011;75(4):298–307. WOS:000299531100009. pmid:22468028
  30. 30. Juteau P, Tremblay D, Villemur R, Bisaillon JG, Beaudet R. Analysis of the bacterial community inhabiting an aerobic thermophilic sequencing batch reactor (AT-SBR) treating swine waste. Appl Microbiol Biot. 2004;66(1):115–22. WOS:000225046200015.
  31. 31. Clifford RJ, Milillo M, Prestwood J, Quintero R, Zurawski DV, Kwak YI, et al. Detection of Bacterial 16S rRNA and Identification of Four Clinically Important Bacteria by Real-Time PCR. Plos One. 2012;7(11). ARTN e48558 WOS:000311315300038.
  32. 32. Oh MH, Paek SH, Shin GW, Kim HY, Jung GY, Oh S. Simultaneous Identification of Seven Foodborne Pathogens and Escherichia coli (Pathogenic and Nonpathogenic) Using Capillary Electrophoresis-Based Single-Strand Conformation Polymorphism Coupled with Multiplex PCR. J Food Protect. 2009;72(6):1262–6. WOS:000266956000013.
  33. 33. Castillo M, Martin-Orue SM, Manzanilla EG, Badiola I, Martin M, Gasa J. Quantification of total bacteria, enterobacteria and lactobacilli populations in pig digesta by real-time PCR. Vet Microbiol. 2006;114(1–2):165–70. WOS:000236745800019. pmid:16384658
  34. 34. Matsuki T, Watanabe K, Fujimoto J, Kado Y, Takada T, Matsumoto K, et al. Quantitative PCR with 16S rRNA-Gene-targeted species-specific primers for analysis of human intestinal bifidobacteria. Appl Environ Microb. 2004;70(1):167–73. WOS:000188115300021.
  35. 35. Sanschagrin S, Yergeau E. Next-generation Sequencing of 16S Ribosomal RNA Gene Amplicons. Jove-J Vis Exp. 2014;(90). ARTN e51709 WOS:000349299200040.
  36. 36. Schloss PD, Westcott SL, Ryabin T, Hall JR, Hartmann M, Hollister EB, et al. Introducing mothur: Open-Source, Platform-Independent, Community-Supported Software for Describing and Comparing Microbial Communities. Appl Environ Microb. 2009;75(23):7537–41. WOS:000271944800028.
  37. 37. Huse SM, Welch DM, Morrison HG, Sogin ML. Ironing out the wrinkles in the rare biosphere through improved OTU clustering. Environ Microbiol. 2010;12(7):1889–98. WOS:000280101200009. pmid:20236171
  38. 38. Molatova Z, Skrivanova E, Bare J, Houf K, Bruggeman G, Marounek M. Effect of coated and non-coated fatty acid supplementation on broiler chickens experimentally infected with Campylobacter jejuni. J Anim Physiol an N. 2011;95(6):701–6. WOS:000297014500003.
  39. 39. Grilli E, Vitari F, Domeneghini C, Palmonari A, Tosi G, Fantinati P, et al. Development of a feed additive to reduce caecal Campylobacter jejuni in broilers at slaughter age: from in vitro to in vivo, a proof of concept. J Appl Microbiol. 2013;114(2):308–17. WOS:000313723800003. pmid:23110383
  40. 40. Hermans D, Martel A, Van Deun K, Van Immerseel F, Heyndrickx M, Haesebrouck F, et al. The Cinnamon-Oil Ingredient trans-Cinnamaldehyde Fails To Target Campylobacter jejuni Strain KC 40 in the Broiler Chicken Cecum Despite Marked In Vitro Activity. J Food Protect. 2011;74(10):1729–34. WOS:000296077400021.
  41. 41. Videnska P, Sisak F, Havlickova H, Faldynova M, Rychlik I. Influence of Salmonella enterica serovar Enteritidis infection on the composition of chicken cecal microbiota. Bmc Vet Res. 2013;9. Artn 140 WOS:000322043900001.
  42. 42. Stanley D, Keyburn AL, Denman SE, Moore RJ. Changes in the caecal microflora of chickens following Clostridium perfringens challenge to induce necrotic enteritis. Vet Microbiol. 2012;159(1–2):155–62. WOS:000308121500020. pmid:22487456
  43. 43. Johansen CH, Bjerrum L, Finster K, Pedersen K. Effects of a Campylobacter jejuni infection on the development of the intestinal microflora of broiler chickens. Poultry Sci. 2006;85(4):579–87. WOS:000236484300001.
  44. 44. Sofka D, Pfeifer A, Gleiss B, Paulsen P, Hilbert F. Changes within the intestinal flora of broilers by colonisation with Campylobacter jejuni. Berl Munch Tierarztl. 2015;128(3–4):104–10. WOS:000351017800004.
  45. 45. Kaakoush NO, Sodhi N, Chenu JW, Cox JM, Riordan SM, Mitchell HM. The interplay between Campylobacter and Helicobacter species and other gastrointestinal microbiota of commercial broiler chickens. Gut Pathog. 2014;6. Artn 18 WOS:000337490900001.
  46. 46. Skanseng B, Kaldhusdal M, Rudi K. Comparison of chicken gut colonisation by the pathogens Campylobacter jejuni and Clostridium perfringens by real-time quantitative PCR. Mol Cell Probe. 2006;20(5):269–79. WOS:000239897300002.
  47. 47. Line JE, Hiett KL, Guard-Bouldin J, Seal BS. Differential carbon source utilization by Campylobacter jejuni 11168 in response to growth temperature variation. J Microbiol Meth. 2010;80(2):198–202. WOS:000275032300014.
  48. 48. Morotomi M, Nagai F, Watanabe Y. Description of Christensenella minuta gen. nov., sp nov., isolated from human faeces, which forms a distinct branch in the order Clostridiales, and proposal of Christensenellaceae fam. nov. Int J Syst Evol Micr. 2012;62:144–9. WOS:000300136200025.
  49. 49. Duncan SH, Hold GL, Harmsen HJM, Stewart CS, Flint HJ. Growth requirements and fermentation products of Fusobacterium prausnitzii, and a proposal to reclassify it as Faecalibacterium prausnitzii gen. nov., comb. nov. Int J Syst Evol Micr. 2002;52:2141–6. WOS:000179838100034.
  50. 50. Hansen AK, Hansen CHF, Krych L, Nielsen DS. Impact of the gut microbiota on rodent models of human disease. World J Gastroentero. 2014;20(47):17727–36. WOS:000346712800004.
  51. 51. Duncan SH, Holtrop G, Lobley GE, Calder AG, Stewart CS, Flint HJ. Contribution of acetate to butyrate formation by human faecal bacteria. Brit J Nutr. 2004;91(6):915–23. WOS:000222418800013. pmid:15182395
  52. 52. Van Deun K, Pasmans F, Van Immerseel F, Ducatelle R, Haesebrouck F. Butyrate protects Caco-2 cells from Campylobacter jejuni invasion and translocation. Brit J Nutr. 2008;100(3):480–4. WOS:000259677300003. pmid:18275629
  53. 53. Wrzosek L, Miquel S, Noordine ML, Bouet S, Chevalier-Curt MJ, Robert V, et al. Bacteroides thetaiotaomicron and Faecalibacterium prausnitzii influence the production of mucus glycans and the development of goblet cells in the colonic epithelium of a gnotobiotic model rodent. Bmc Biol. 2013;11. Artn 61 WOS:000319910600001.
  54. 54. Mookiah S, Sieo CC, Ramasamy K, Abdullah N, Ho YW. Effects of dietary prebiotics, probiotic and synbiotics on performance, caecal bacterial populations and caecal fermentation concentrations of broiler chickens. J Sci Food Agr. 2014;94(2):341–8. WOS:000328058900024.
  55. 55. Ding W, Wang HF, Griffiths MW. Problotics down-regulate flaA sigma(28) promoter in Campylobacter jejuni. J Food Protect. 2005;68(11):2295–300. WOS:000233096200006.
  56. 56. Santini C, Baffoni L, Gaggia F, Granata M, Gasbarri R, Di Gioia D, et al. Characterization of probiotic strains: An application as feed additives in poultry against Campylobacter jejuni. Int J Food Microbiol. 2010;141:S98–S108. WOS:000281830700013. pmid:20452074
  57. 57. Messier S, Quessy S, Robinson Y, Devriese LA, Hommez J, Fairbrother JM. Focal Dermatitis and Cellulitis in Broiler-Chickens—Bacteriological and Pathological Findings. Avian Dis. 1993;37(3):839–44. WOS:A1993LY02100031. pmid:8257380
  58. 58. Tiihonen K, Kettunen H, Bento MHL, Saarinen M, Lahtinen S, Ouwehand AC, et al. The effect of feeding essential oils on broiler performance and gut microbiota. Brit Poultry Sci. 2010;51(3):381–92. Pii 925013654 WOS:000280517400009.
  59. 59. Cross DE, McDevitt RM, Hillman K, Acamovic T. The effect of herbs and their associated essential oils on performance, dietary digestibility and gut microflora in chickens from 7 to 28 days of age. Brit Poultry Sci. 2007;48(4):496–506. WOS:000248722000012.
  60. 60. Boroojeni FG, Vahjen W, Mader A, Knorr F, Ruhnke I, Rohe I, et al. The effects of different thermal treatments and organic acid levels in feed on microbial composition and activity in gastrointestinal tract of broilers. Poultry Sci. 2014;93(6):1440–52. WOS:000337078000015.