The skin is inhabited by a multitude of microorganisms. An imbalance of these microorganisms is associated with disease, however, the causal relationship between skin microbiota and disease remains unknown. To describe the cutaneous bacterial microbiota of cats and determine whether bacterial dysbiosis occurs on the skin of allergic cats, the skin surfaces on various regions of 11 healthy cats and 10 allergic cats were sampled.
Genomic DNA was extracted from skin swabs and sequenced using primers that target the V4 region of the bacterial 16S rRNA. The bacterial sequences from healthy cats revealed that there are differences in species diversity and richness between body sites and different epithelial surfaces. Bacterial communities preferred body site niches in the healthy cats, however, the bacterial communities on allergic cat skin tended to be more unique to the individual cat. Overall, the number of bacterial species was not significantly different between the two health status groups, however, the abundances of these bacterial species were different between healthy and allergic skin. Staphylococcus, in addition to other taxa, was more abundant on allergic skin.
Citation: Older CE, Diesel A, Patterson AP, Meason-Smith C, Johnson TJ, Mansell J, et al. (2017) The feline skin microbiota: The bacteria inhabiting the skin of healthy and allergic cats. PLoS ONE 12(6): e0178555. https://doi.org/10.1371/journal.pone.0178555
Editor: Marie-Joelle Virolle, Universite Paris-Sud, FRANCE
Received: November 9, 2016; Accepted: May 15, 2017; Published: June 2, 2017
Copyright: © 2017 Older et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All of the original sequence files are available from the SRA database under the SRA study id: SRP091923 at https://trace.ncbi.nlm.nih.gov/Traces/sra/sra.cgi?study=SRP091923.
Funding: Funding was provided by the Winn Feline Foundation (http://www.winnfelinefoundation.org/) under grant ID MT14-018. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
The body is colonized by a variety of microorganisms. These microorganisms can be beneficial, by educating the immune system and inhibiting the growth of pathogenic microorganisms, or they can be pathogenic, producing disease in affected tissues [1, 2]. The microbial populations present in and on the body vary with different anatomical locations [2, 3]. Likewise, they differ between individuals due to intrinsic and extrinsic factors, such as immune status and environment, respectively. Some studies have shown that molecular or cellular alterations in the skin [4, 5] and intestinal tract [6, 7] have an effect on the composition of the microbiota, however it is still unclear if changes in the cutaneous microbiota are triggered by disease or result in disease [2, 8]. Regardless, it appears that there is a relationship between alterations in the skin microbiota and disease [1, 9]. By studying the microbiota of skin in healthy individuals, a standard is set for what is “normal”, which can subsequently be used to understand how differences in these opportunistic microorganisms may be causing or contributing to infections or disease [2, 9].
Several studies have been performed to describe the microbiota of various body regions in humans, including the skin [2, 3, 10]. In veterinary medicine, fewer studies regarding the microbiota in animals have been performed, however this is a growing area of important research. There have been several studies describing the gastrointestinal [11–13] and oral microbiota of cats and dogs [14–18]. In the oral cavity of cats, Sturgeon et al. found a predominance of unidentified Pasteurellaceae, Moraxella, Thermomonas, and unclassified Comamonadaceae . In dogs, they found Porphyromonas dominating the oral cavity . A few studies have been conducted on the cutaneous microbiota of animals [9, 19–22]. In dogs, the cutaneous bacterial microbiota belongs to the phyla Proteobacteria, Actinobacteria and Firmicutes . One study looked at how the microbiota in dogs change with atopic flares and treatments, and found that treatment results in normalization of the bacterial communities . Dogs with allergic skin disease, such as atopic dermatitis (AD), are colonized by a different microbiota than healthy dogs [9, 19, 23, 24].
Studies have also looked at how the microbiota is shared between animals and their owners [14, 15, 18, 25]. Song et al. found that the skin microbiota of adults who own dogs are more similar to that of other dog owners than non-dog owning adults. Some results have indicated that living with cats and/or dogs, and thus sharing microbiotas, can help reduce the risk of developing allergies in people [26, 27]. However, the data for cat ownership is still conflicting [26, 28–30]. Current studies show that cat ownership could result in decreased  or increased [26, 29, 30] allergies in children, and some studies have failed to find any correlation between children allergies and cat ownership .
Although the human and canine skin microbiota has been described in multiple studies, the feline skin microbiota remains somewhat unknown. Most of the recent research on the skin microbiota of cats has focused on Staphylococcus due to its role in skin diseases [33, 34]. Previously, a culture based study was performed with the goal of describing the feline skin microbiota and found that Micrococcus, Acinetobacter, Streptococci, and Staphylococci dominated the sites sampled; however, bacteria could not be isolated from half of the samples, which the authors attributed to the normal grooming behavior of cats . Recent studies have also examined the fungal mycobiota in healthy and allergic cats and dogs, which have found significant differences in the fungal communities colonizing the skin [20, 21].
The objectives of this study were to describe the bacterial microbiota present on different skin surfaces of healthy cats and identify differences between healthy cats and cats with allergic skin disease. We hypothesized that next-generation sequencing of feline skin swabs would reveal a preference of specific bacterial microbiota to different body sites. Furthermore, we expected to see differences in the diversity and specific bacterial taxa present on the skin of allergic cats compared to those without skin disease.
Materials and methods
This study had been approved by the Texas A&M University (TAMU) Institutional Animal Care and Use Committee under 2012–139. Informed consent to enroll clinical cases into the study was obtained from each client.
Collection of samples from all animals enrolled in this study followed a protocol approved by the Texas A&M University Institutional Animal Care and Use Committee.
Eleven healthy cats participated in this study with their ages ranging from 2 to 17 years old (Table 1). Included were 6 spayed females (3 domestic shorthairs (DSH), 1 domestic medium hair (DMH), 2 domestic long hairs (DLH)) and 5 neutered males (3 DSH, 1 DMH, 1 DLH). All of these cats lived with other animals. Six of the cats were kept indoors, three spent time both inside and outside, and one was kept solely outdoors. All cats were evaluated by a board certified dermatologist, and none had skin lesions, history of pruritus or any history of skin disease in the past 6 months. These patients were not treated with antibiotics, antifungals, anti-inflammatory or immunosuppressive drugs for at least 6 months prior to sample collection. Fleas were not present on any of the cats at the time of sample collection.
Ten cats with allergic skin disease were enrolled in this study with ages ranging from 5 to 11 years old (Table 1). Included were 5 spayed females (4 DSH and 1 Siamese), 1 intact female (DSH), 3 castrated males (2 DSH and 1 Siamese), and 1 intact male (Persian). All but two of these cats lived with or had contact with other animals. Six of the cats were kept indoors and four spent time both inside and outside. All allergic cats were evaluated by a board certified veterinary dermatologist. Allergic cats in this study were defined as those with a history of pruritus/over-grooming and/or that showed common cutaneous reaction patterns (self-induced alopecia, miliary dermatitis, eosinophilic skin lesions, and/or cervicofacial dermatitis). All parasitic and infectious causes of pruritus had been ruled out by standard diagnostic and therapeutic methods. Allergic cats included animals with flea allergy dermatitis, cutaneous adverse food allergies, and feline non-flea non-food hypersensitivity reactions and were allowed to be maintained clinically on various medications according to their specific disease (e.g. adulticidal flea prevention, hypoallergenic diet, anti-inflammatory medications, allergen-specific immunotherapy). None of the cats presented with flea or ear problems. Three cats (F16, F18, F19) were treated with antibiotics prior to the study, however not within at least 1 month of sample collection.
Skin swabs were collected from 12 sites from the healthy cats: axilla, chin, conjunctiva, dorsal nose, ear canal, groin, interdigital skin, lumbar region, nostril, oral cavity, pinna, and reproductive tract (prepuce or vulva). Skin swabs were collected from 6 sites from the allergic cats: axilla, ear canal, groin, interdigital skin, lumbar region, and nostril. Three Isohelix buccal swabs (Cell Projects Ltd., Kent, UK) were used per skin site. Each side of the swab was rubbed on the skin 10 times. Two swabs were collected in a MoBio PowerBead tube with 750 μl buffer containing guanidine thiocyanate as well as additional proprietary reagents (MoBio Laboratories, Carlsbad, CA). Buffers containing guanidine thiocyanate have been previously described to preserve nuclei acids in field samples for up to 41 days without refrigeration . Another swab was added to a 2 ml collection tube without any reagents. All samples were immediately stored for no longer than 30 days at 4°C until extractions were performed.
DNA extraction and sequencing
Genomic DNA was extracted from skin swabs using the MoBio PowerSoil DNA Isolation Kit according to the manufacturer’s protocol. Extractions were also performed on unused Isohelix buccal swabs and empty PowerBead tubes to serve as negative controls. Extracted DNA and control samples were sequenced on an Illumina MiSeq instrument at the University of Minnesota Genomics Center using forward primer 515F: GTGYCAGCMGCCGCGGTAA and reverse primer 806R: GGACTACNVGGGTWTCTAAT that target the 16S rRNA gene .
The raw sequences were processed using QIIME v1.9.1  to perform quality filtering, definition of operational taxonomic units (OTUs) (sequences with 97% similarity) , and taxonomic classification with the Greengenes database [39–42]. Suspected contaminants found in the controls were removed by filtering them from the OTU table as previously described . For the purpose of comparing different physiologies of the sites sampled, the chin was considered “sebaceous”; the axilla, dorsal nose, ear canal, groin, interdigital, lumbar, and pre-aural space were considered “haired skin”; the conjunctiva, nostril, and reproductive were considered “mucosal” or “mucocutaneous junctions”; and the oral cavity was considered unique and referred as “oral”. Alpha diversity (number of bacterial species) was calculated using Chao1, Shannon, and observed OTUs metrics to determine species richness and evenness of each sample. Beta diversity (bacterial community composition) was calculated using weighted UniFrac, unweighted UniFrac, and Bray-Curtis metrics to measure similarity between samples; resulting plots were viewed using EMPeror .
The analysis of similarities (ANOSIM) function of PRIMER 7 (PRIMER-E Ltd., Luton, UK) was performed on the distance matrices from beta diversity calculations to assess differences in bacterial community composition. A Kruskal-Wallis test was performed using JMP Pro 11 (SAS Institute Inc., Cary, NC) to assess differences in the alpha diversity and relative abundance of bacterial taxa. P-values were corrected for false discovery rate, as previously described . The relative abundance tables were filtered and linear discriminant analysis (LDA) effect size (LEfSe) performed with an alpha value of 0.01 to analyze the difference in taxa abundance with the different variables (cat number, body site, physiology, health condition) .
From the 192 samples from healthy and allergic cats, 5 samples (2 from healthy cats, 3 from allergic cats) were excluded from the analysis due to low sequence counts. Seven taxa (Xanthomonadaceae, 0319-6G20, Comamonadaceae, Beijerinckiaceae, Thermoactinomycetaceae, Weeksellaceae, and unassigned Rhizobiales) were very abundant in the negative control samples. These taxa and Cyanobacteria were filtered out of the OTU tables prior to downstream analysis .
The OTU table was rarefied to 3100 sequences. The average number of sequences per sample was 34378. A total of 8137 OTUs were identified with 31 resulting phyla (S4 Table).
Species richness and diversity.
The samples from the healthy cats were compared based on cat number, body site, and physiology of the different sites. The three alpha diversity metrics used included Shannon, Chao1 and observed OTUs (Table 2). Observed OTUs gives insight into the richness of the microbial communities present, Chao1 estimates richness at full sequencing coverage, while Shannon takes into account richness and evenness. The pre-aural space was the site with the greatest richness and even distribution of these species, while the mucosal sites (reproductive, nostril, and conjunctiva) and ear canal had the lowest alpha diversity (Fig 1). Out of the skin physiologies compared (haired, mucosal, oral, and sebaceous), haired skin had the highest richness and evenness, while mucosal surfaces had the lowest (S1 Fig). Kruskal-Wallis tests revealed that all three alpha diversity metrics resulted in significant differences in the number of observed OTUs and the richness of the populations present when comparing individual cats, different body sites, and different physiologies (S1 Table).
Results from pairwise Kruskal-Wallis tests on body sites in healthy cats at a rarefaction of 3100 sequences per sample. Asterisks indicate sites that were found to be significantly different from at least 8 other body sites.
Microbial community structure.
Beta diversity measures (weighted UniFrac, unweighted UniFrac, and Bray-Curtis) indicated that body site had an impact on difference in community structure between samples (S2 Table). All three beta diversity metrics showed significance in dissimilarity when comparing the different sites sampled overall (R = 0.278, R = 0.252, R = 0.343 respectively, all with p = 0.001) (Fig 2) and with pairwise comparisons (S3 Table). Some clustering was observed when comparing individual cats, however less so than with body site (R = 0.175, R = 0.195, R = 0.209 respectively, with p = 0.001 for all) (Fig 3). Comparing the samples based on physiology of the sampled site resulted in significant differences in community structure based on weighted UniFrac (R = 0.320, p = 0.001) and Bray-Curtis (R = 0.297, p = 0.001) beta diversity measures. However, the chin, which was analyzed as the sebaceous site, did not cluster differently from the haired sites (S2 Fig).
Principal coordinate analysis plots of weighted UniFrac, unweighted UniFrac, and Bray-Curtis distance matrices. Significant clustering was seen with all three measures of beta diversity.
ANOSIM of beta diversity distance matrices resulted in the shown R values. R values range from -1 to 1, with values closer to 0 indicating compared groups are very similar. Allergic cats clustered most by individual cat while healthy cats clustered most by body site.
Microbial community composition.
Overall, the most common phyla in cats were found to be Proteobacteria (46.4%), followed by Bacteroidetes (20.7%), Firmicutes (17.7%), Actinobacteria (8.6%), and Fusobacteria (4.1%) (Fig 4). The most common families sequenced were Porphyromonadaceae, Moraxellaceae, Pasteurellaceae, and Pseudomonadaceae. Using a pairwise Kruskal-Wallis test, we found that many taxa were significantly different in abundance based on physiology, body site, and/or individual cat. Differential taxa abundance was also seen between female and male cats at the reproductive site (S3 Fig). LEfSe did not reveal any significant differences in taxa abundances between cats, body sites, or physiologies.
Average relative taxa abundances at each body site (axilla, chin, conjunctiva, dorsal nose, ear canal, groin, interdigital, lumbar, nostril, oral, pre-aural space, and reproductive organs) sampled in healthy cats. Four phyla (Proteobacteria, Bacteroidetes, Firmicutes, and Actinobacteria) accounted for 97.5% of the bacteria found in the samples.
The OTU table was rarefied to 2900 sequences. The average number of sequences per sample was 36490. A total of 4374 OTUs were identified with 19 resulting phyla.
Species richness and diversity.
All alpha diversity metrics (Chao1, Shannon, observed OTUs) indicated significant differences between individual cats (p = 0.0354, p = 0.0231, and p = 0.0051 respectively) (Table 3). When comparing the two physiologies of the sites sampled in the allergic cats (haired skin and mucosal), the Shannon index showed significant differences in evenness with p = 0.0103. No significance in alpha diversity was seen when comparing the body sites sampled overall, however some significance was found in pairwise comparison tests.
Microbial community structure.
Community structure differed significantly between cats, according to the beta diversity metrics used (weighted UniFrac = 0.396, unweighted = 0.49, Bray-Curtis = 0.54, all with p = 0.001) (Fig 5). Community structure also differed by physiology of the sampled site (haired or mucosal) according to weighted UniFrac and Bray-Curtis (R = 0.230, R = 0.280 respectively, with p = 0.001). Unlike the samples from healthy cats, samples from allergic cats did not cluster by body site.
Microbial community composition.
The most common phyla in allergic cats were found to be Proteobacteria (49.0%) followed by Firmicutes (21.5%), Actinobacteria (13.7%), Bacteroidetes (11.2%), and Fusobacteria (3.0%). The most abundant families were Pseudomonadaceae, Moraxellaceae, Pasteurellaceae, and Neisseriaceae. The haired sites sampled (axilla, ear canal, groin, interdigital, lumbar) had more Firmicutes, specifically Clostridiales. LEfSe revealed that the mucosal site sampled (nostril) had more Corynebacterium and that 5 of the cats had taxa communities that were very different than all of the other cats (S4 Fig).
Skin microbiota of healthy versus allergic cats
The samples used in the analysis to compare healthy and allergic cats included swabs from the axilla, ear canal, groin, interdigital, lumbar, and nostril. The OTU table was rarefied to 2900. The average number of sequences per sample was 35850. A total of 7100 OTUs were identified resulting in 23 phyla.
Species richness and diversity.
The results for alpha diversity are shown in Table 4. No significant differences were found in species richness and diversity between healthy and allergic cats overall. A significant difference was found between the allergic and healthy nostril with Chao1 (p = 0.02).
Microbial community structure.
A significant difference in overall community composition was not found between healthy and allergic cats. However, with the Bray-Curtis metric, the ear canal did show unique clustering between healthy and allergic skin (R = 0.223, p = 0.014) (S5 Fig).
Microbial community composition.
Fig 6. shows the relative abundances of the bacteria on the sites sampled from both healthy and allergic skin. Using Kruskal-Wallis tests, we discovered that many bacteria were differentially abundant on healthy and allergic skin. At the family level, healthy cats had more Oxalobacteraceae (p<0.0001), Alicyclobacillaceae (p<0.0001), Sphingobacteriaceae (p = 0.0023), and Chitinophagaceae (p = 0.0324), while allergic cats had more Bradyrhizobiaceae (p = 0.0080), Prevotellaceae (p = 0.0205), Vibrionaceae (p = 0.0310), and Halomonadaceae (p = 0.0023) (S4 Table).
A. Average relative taxa abundances at each body site (axilla, ear canal, groin, interdigital, lumbar, and nostril) sampled in healthy and allergic cats. B. Individual relative taxa abundances in every site sampled in healthy and allergic cats.
LEfSe demonstrated that overall, healthy cats had more Oxalobacteraceae and Porphyromonadaceae, and allergic cats had more Staphylococcus (Fig 7). When looking at the different body sites separately, LEfSe also revealed differences in relative taxa abundance between healthy and allergic cats, including increased Oxalobacteraceae in healthy cats at multiple sites (S6 Fig).
In this study we demonstrated that the bacterial microbiota on the skin of healthy cats tends to prefer specific body site niches and skin physiologies (haired, mucosal, sebaceous, and oral). The bacteria colonizing the skin also varies between individual cats, however, less so than between different sites and types of regions sampled. In dogs, high variability was seen between individuals, but a similar microbiota was seen with respect to some of the body sites sampled .
We found the same phyla that were most abundant on the skin of dogs  were also the most abundant on feline skin, however in a different order (Proteobacteria, followed by Bacteroidetes, Firmicutes, and Actinobacteria). Bacteria of the phyla Bacteroidetes were highly abundant in all sites of the sampled cats, compared to what has been previously found in dogs . This difference in Bacteroidetes abundance, a phyla typically associated with the oral cavity, may be due to the grooming behavior of cats.
When comparing specific body sites, ear canal, conjunctiva, nostril, and reproductive tracts had the least amount of observed OTUs and relatively low evenness. When considering the different physiologies of the sites sampled, haired and sebaceous sites were the most rich and diverse, followed by oral and mucosal. This is similar to what was found in dogs, where the haired sites had a higher species richness than mucosal surfaces and mucocutaneous junctions . The diversity and richness was in the median range for canine ear canal, however in cats, the ear canal was one of the sites with relatively low diversity and richness.
Significant differences in the relative abundance of specific bacteria between healthy and allergic feline skin were identified (Fig 7). In the allergic cats, there were higher proportions of Staphylococcus which has been associated with atopic dermatitis in humans and dogs [19, 23, 46]. Although previous studies have indicated that Staphylococcus skin infections are less common in cats [47–50], possibly due to decreased adherence to corneocytes [33, 34], our finding indicates there may be a relationship between allergic skin disease and the increased abundance of Staphylococcus in cats.
Healthy and allergic cats also showed differences in community structure; samples from healthy cats clustered most by body site, whereas samples from allergic cats clustered most by individual cat. Additionally, the ear canal, a site often affected in hypersensitivity reactions , showed significant clustering between healthy and allergic cats. This shift may support the idea that there is a “normal” bacterial microbiota that is disrupted when an animal develops allergic skin disease. Instead of having a community unique to each site, with skin allergy flare ups, cats may become colonized all over the body by a single altered community. This change in the bacterial communities of all body sites, instead of just the affected area, may be reflective of the grooming behavior of cats. Every clinical presentation of a disease can be slightly different (e.g., different cutaneous reaction patterns), and similarly there does not seem to be one standard “unhealthy” microbiota.
Although this study may support the relationship between the bacterial microbiota and disease, the bacterial communities may not be the only ones affected by or contributing to disease. Studies on the fungal mycobiota have already looked for differences between animals with and without skin diseases. Meason-Smith et al. found that dogs most clustered by individual, regardless of health condition . This same clustering by individual, regardless of health, was also seen in a similar study done on cats . In both studies, differences in relative taxa abundance between healthy and allergic animals were identified. Overall, it seems that fungi on the skin of cats  and dogs  clusters mostly by individual animal, whereas bacteria seem to cluster mostly by body site .
One of the limitations of this study was the primer set used. It has previously been found that the primers we used to sequence the V4 region of the 16S rRNA are unable to amplify the genus Propionibacterium  due to a single mistmatch . Although the primer set used in the presented study is not able to successfully amplify Propionibacterium spp., the primer set is able to amplify other bacteria, which cannot be amplified by other primer sets that have some relevance to the human skin microbiota . However, studies comparing the effectiveness of different 16s rRNA gene primer sets in amplifying bacteria relevant to the feline skin microbiota have not yet been performed. This current study only identified very low abundances of the genus Propionibacterium, but future studies utilizing different primers may show the genus Propionibacterium to be more abundant than described in the current study and may reveal different relative abundances for other taxa.
Another limitation of this study was the small sample size used in the two groups and the heterogeneity of the feline population included in the study. We aimed to obtain as much homogeneity for certain factors in our sample cohort as possible by including approximately equal numbers of spayed females and neutered males. Most cats included in this study were domestic short hairs, the main breed in the general feline population. Obtaining homogeneous animal populations can be difficult, and doing so would limit the sample size included in this study even more. One way of overcoming heterogeneity of the sample cohort would be by including a homogenous feline research colony. Animals in research colonies are not exposed to typical household environments and often belong to a single breed through, so would not be representative of the general feline population, which was the goal of this study.
Currently, there is very little known about the feline skin bacterial microbiota . Our study revealed that there are many more bacterial species found on feline skin than previously thought. It is important that at this point, results obtained with this first study be interpreted as descriptive and that additional follow up studies including larger sample sizes be repeated to support these findings. Furthermore, confounding factors, such as breed, sex and environment, that could influence the composition of the skin microbiota should be evaluated separately. Using other molecular techniques will allow for validation of these results and may reveal more about the microbiota than can be demonstrated with either next-generation sequencing or culture based methods. Evaluation of the changes in the microbiota with flares of disease and treatment may also help elucidate more about the relationship between cats and their microbiota.
S1 Table. Alpha diversity averages at 3100 sequences per sample for healthy cats.
Values represent averages with standard deviations in parenthesis. Superscript letters represent sites that were significantly different according to Kruskal-Wallis tests with p<0.05.
S2 Table. Global R statistics for beta diversity analysis.
S3 Table. R statistics for significant (R≥ 0.200, p≤0.05) pairwise comparisons.
Shown R values are averages and p-values are ranges from pairwise comparisons. No significant pairwise comparisons in allergic samples with body site.
S4 Table. Filtered relative taxa abundances and results from Kruskal-Wallis tests for differential taxa abundance.
P-values ≤ 0.05 are in bold. Median (Min-Max).
S5 Table. Hypersensitivity information (type, age of onset, seasonality, clinical signs, lesion distribution, ear problems, and treatments for ten allergic cats.
Allergy treatments were concurrent. All cats with a Y in the steroids column had previously received steroids, except for F14 and F15 that were receiving steroids at the time of sampling. F18 was diagnosed with a ringworm infection, treated with limed dips, and lesions resolved three months prior to sample collection.
DSH-Domestic short hair, Per-Persian, Sia-Siamese, FBH-Flea bite hypersensitivity, FIHD-Food induced hypersensitivity, NFNFIHD- Non-flea non-food induced hypersensitivity, NFBH- non-flea bite hypersensitivity, G-gradual, Y-Yes, N-No. Modified from Meason-Smith C, Diesel A, Patterson AP, Older CE, Johnson TJ, Mansell JM, et al. Characterization of the cutaneous mycobiota in healthy and allergic cats using next generation sequencing. Vet Dermatol. 2016:1–11.
S1 Fig. Alpha diversity plots of the physiologies sampled in healthy cats.
P-values are from Kruskal-Wallis tests. Lines indicate pairwise comparisons that resulted in significant p-values.
Principal coordinate analysis plots of Weighted UniFrac distance matrices of healthy cat samples by A. individual cat and B. physiology.
S3 Fig. Average relative taxa abundances in the reproductive samples from healthy cats.
S4 Fig. LEfSe plots and cladograms from allergic cat samples.
S5 Fig. Principal coordinate analysis plot of healthy vs. allergic ear canal.
Principal coordinate analysis plot based on Bray-Curtis distance matrix comparing healthy and allergic ear canal samples. Healthy and allergic ear canal samples showed distinct clustering.
We would like to thank Amanda Friedrick for assistance with sample collection, Dr. Kimberly Wahl for assistance with DNA extractions, and the cats and their owners for participation in this study.
- Conceptualization: AD APP JM JSS ARH.
- Data curation: CEO ARH.
- Formal analysis: CEO CMS JSS ARH.
- Funding acquisition: AD APP JSS ARH.
- Investigation: CEO AD APP CMS TJJ ARH.
- Methodology: CEO ARH.
- Project administration: ARH.
- Resources: AD APP JM JSS ARH.
- Supervision: ARH.
- Visualization: CEO ARH.
- Writing – original draft: CEO ARH.
- Writing – review & editing: CEO AD APP CMS TJJ JM JSS ARH.
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