Journal of Biomedical Translational Research
Research Institute of Veterinary Medicine, Chungbuk National University
Original Article

Alteration of goat kids’ gut microbiota by Cryptosporidium parvum infection

Subin Lee1, Badriah Alkathiri1, Ah-Young Kim2,3, Kyung-Hyo Do1, Kwangwon Seo1,2, Soochong Kim1,2, Wan-Kyu Lee1,2, Dongmi Kwak4, Seung-Hun Lee1,2,*
1College of Veterinary Medicine, Chungbuk National University, Cheongju 28644, Korea
2Graduate of Veterinary Biosecurity and Protection, Chungbuk National University, Cheongju 28644, Korea
3Department of Animal Health, Agricultural Policy Bureau, Chungbuk Provincial Government, Cheongju 28515, Korea
4College of Veterinary Medicine, Kyungpook National University, Daegu 41566, Korea
*Corresponding author: Seung-Hun Lee, College of Veterinary Medicine, Chungbuk National University, Cheongju 28644, Korea, Tel: +82-43-261-3892, E-mail:

© Research Institute of Veterinary Medicine, Chungbuk National University.

Received: Apr 24, 2024; Revised: May 24, 2024; Accepted: May 28, 2024


Caprine cryptosporidiosis mainly occurs in young goats, with morbidity rates of 80%–100% and mortality over 50% in goat kids. However, limited research has been conducted on the impact of Cryptosporidium parvum, a diarrhea-causing pathogen, on the intestinal microbiota of goat kids. In this study, 16S rRNA-based metataxonomic analysis was performed to compare the microbial diversity and abundance of the gut microbiota between C. parvum-infected and uninfected goat kids. In total, 12 goat fecal samples were collected, including seven naturally C. parvum-infected and five uninfected goats from Chungcheongbuk-do, Korea. After amplification of the V3–V4 hypervariable region of the bacterial 16S rRNA, high-throughput sequencing was performed. The results showed differences in the microbial composition between C. parvum-infected and uninfected groups based on beta diversity. Firmicutes and Bacteroidetes were the most dominant phyla in both groups. However, no significant difference was observed in the Bacteroidetes/Firmicutes ratio between the two groups. Compared with the uninfected group, the C. parvum-infected group showed significantly higher abundances of Tyzzerella nexillis, Lactobacillus johnsonii, Butyricicoccus pullicaecorum, Enterococcus raffinosus, Enterococcus faecalis, and Negativicoccus massiliensis, and significantly reduced abundances of Aerococcus vaginalis, Faecalicoccus pleomorphus, Oribacterium parvum, and Coprococcus comes. These findings indicate that C. parvum infection, which is associated with diarrhea in neonatal goats, induces alterations in the caprine gut microbiota.

Keywords: Cryptosporidium parvum; gastrointestinal microbiome; goat; 16S rRNA; next-generation sequencing


Cryptosporidium parvum is an obligate intracellular apicomplexan protozoon that infects the small intestine. Cryptosporidium is globally distributed and infects a wide range of hosts including livestock, poultry, and humans, and forms an important aspect of public health. Cryptosporidiosis, caused by C. parvum, disrupts the small intestinal villi and epithelial cells, leading to mucosal inflammation and a reduction in enzymatic activity [1]. This disruption results in compromised intestinal mucosal barriers, increased intestinal permeability, and the secretion of fluids and electrolytes, leading to dysfunctional digestion and absorption [2]. Consequently, the clinical symptoms of cryptosporidiosis vary from watery diarrhea, weight loss, poor growth performance, and decreased feed efficiency to life-threatening conditions, especially in immunodeficient and neonatal animals [3].

Caprine cryptosporidiosis mainly occurs in young animals (< 2 months old), and infected goat kids excrete a large number of oocysts (107–108 oocysts per gram) [4]. Cryptosporidiosis in adult goats is generally asymptomatic because of the host’s strong immune response; however, it exhibits 80%–100% morbidity and > 50% mortality in goat kids [5]. Therefore, controlling cryptosporidiosis is of great interest to the small ruminant industry. However, no effective drug or vaccine is currently available; instead, only sanitary management and supportive therapies such as rehydration, feed supplementation, and antidiarrheal agents have been employed.

Goats, as ruminants, possess a complex and distinctive digestive system that is well-suited for fermentation. Gut microorganisms present in ruminants play a pivotal role in the breakdown of plant fibers, significantly contributing to energy production [6]. These microorganisms generate up to 70% of the daily host enzyme requirements. Additionally, the gut microbiota actively stimulated villus growth in the rumen wall, demonstrating its impact on the overall digestive process [7]. Previous studies have shown that the structure and relative abundance of the caprine gut microbiota are affected by dietary changes, acquisition of colostrum and milk, the physiological environment of the gut, and administration of antibiotics [7-11].

Scientific interest in the association between parasitic infections and gut microbiota in animals is increasing because parasitic infections alter the host gut microbiota diversity and composition, leading to metabolic disorders [12-14]. Parasites infecting the gastrointestinal tract induce functional impairment of the gastrointestinal system, resulting in diarrhea [15]. Goat kids are particularly susceptible to parasitic infections and frequently experience diarrhea. Previous studies have shown that the composition of the ruminant gut microbiota is altered by the occurrence of diarrhea [9, 16]. However, limited research has been conducted on the impact of C. parvum, a diarrhea-causing pathogen, on the intestinal microbiota of goat kids.

Recently, metataxonomic analysis using high-throughput sequencing has been developed and implemented to study alterations in the diversity and composition of the gut microbiota in response to pathogenic infection [17]. This approach can deepen our knowledge of host–parasite interactions and provide alternative ways to control parasitic infections. Therefore, this study aimed to identify the effect of C. parvum infection on gut microbial composition and diversity in goat kids.


Sample collection

In this study, 12 fecal samples were obtained from goat kids (< 1-month-old) on a single goat farm in Chungcheongbuk-do, Korea. Among the 12 fecal samples, seven were naturally infected with C. parvum showing diarrhea and five were from C. parvum-uninfected goat kids. Infection with C. parvum was verified by conventional polymerase chain reaction (PCR) as described in our previous study; however, the presence of other diarrhea causing pathogens was not verified [18]. All goats were raised in an intensive farm system for meat production and were of mixed breed. Information on the diet of goats was not collected.

Diarrheal feces were collected from the rectum using a sterile wooden stick, whereas nondiarrheal feces were collected immediately after defecation. All fecal samples were transported to College of Veterinary Medicine, Chungbuk National University, and stored at 4°C until further processing.

DNA extraction and amplicon-based next-generation sequencing

Genomic DNA was extracted from each fecal sample using the QIAamp® Fast DNA Stool Mini Kit (Qiagen, Hilden, Germany) following the manufacturer’s instructions. DNA quality was assessed using a Qubit 4 Fluorometer (Thermo Fisher Scientific, Waltham, MA, USA), and the DNA was stored at –20℃ until further processing.

The V3–V4 hypervariable region of the bacterial 16S rRNA gene was amplified using locus-specific primers (341F/805R), and sequencing was performed on the Illumina MiSeq platform (Illumina, San Diego, CA, USA) [19]. PCR was conducted in a total reaction volume of 25 μL containing 2.5 μL gDNA, forward and reverse primers (5 μL each; 1 μM), and KAPA HiFi Hotstart ReadyMix (12.5 μL; Kapa Biosystems, Boston, MA, USA) under following conditions: 95℃ initial denaturation for 3 min followed by 25 cycles of 95℃ for 30 s, 55℃ for 30 s and 72℃ for 30 s, and a final extension at 72℃ for 5 min. Nextera XT index adaptors (Illumina) were used for the index PCR. PCR products were purified with AMPure XP beads (Beckman Coulter, Brea, CA, USA). Amplicons were quantified using a Qubit dsDNA HS Quantification Assay (Thermo Fisher Scientific). DNA libraries were multiplexed and sequenced on an Illumina MiSeq system, according to the manufacturer’s instructions.

Sequence processing and amplicon sequence variant table construction

Raw paired-end Illumina sequences were processed using the dada2 pipeline (version 1.28.0) in R software (version 4.3.2) [20]. Briefly, the processes involved primers were trimmed and filtered using the “filterAndTrim” function. Reads exceeding 4 (forward) and 6 (reverse) expected errors based on quality scores were filtered out, and truncation was performed after 280 (forward) and 260 (reverse) base pairs. The dada2 algorithm was applied to infer the exact amplicon sequence variants (ASVs) from the processed sequences, while filtering chimeras. For taxonomic assignment, a naïve Bayesian classifier method was used based on the SILVA reference database (version 138; with a minimum bootstrap confidence of 50. An ASV table was constructed by recording the number of times that each ASV was observed in each sample.

Microbiota analysis with phyloseq

The ASV table, sample data, and taxonomy table were imported into the R environment as “phyloseq” objects (version 1.44.0) [21]. Additional sample data categories were added to the phyloseq sample data table. ASVs without assigned phyla were filtered and agglomerated at the species level. Alpha and beta diversity metrics were calculated on the filtered ASV table using Phyloseq’s estimate_richness and distance functions. Taxonomy summaries and microbial composition bar plots were generated at both phylum and class levels.


Amplicon-based next-generation sequencing data

As a raw data, 1,873,294 pairs of readings (mean: 156,107.83; S.D.: 11,472.82) were obtained. After processing the raw sequences, 1,274,317 (mean: 106,193.08; S.D.: 6,865.77) high-quality read pairs were obtained. In total, 256 ASVs were identified based on the SILVA reference database. The number of ASVs according to the samples varied from 85 to 126 (mean: 108.17; S.D.: 12.14).

Microbial diversity analysis

Alpha diversity indices were used to analyze species richness. The Observed, InvSimpson, Chao1, and abundance-based coverage estimators diversity indices showed no significant differences in the gut microbial biodiversity between C. parvum-infected and uninfected goat kids (p>0.05). However, the Shannon diversity index was statistically significant (p<0.05; Fig. 1A).

Fig. 1. Comparisons of fecal microbial diversity between Cryptosporidium parvum-infected and uninfected groups. (A) Alpha diversity was analyzed using Observed, InvSimpson, Shannon, Chao1, and ACE diversity indices. Based on (B) Bray–Curtis distance, (C) Jaccard distance methods, and (D) pairwise PERMANOVA test (p<0.05), beta diversity revealed significant differences in microbial diversity between the two groups. ACE, abundance-based coverage estimators; PERMANOVA, permutational analysis of variance.
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Beta-diversity analysis was conducted to assess the microbial community composition. In principal coordinate analysis using the Bray–Curtis distance and Jaccard distance methods, samples from the same group were clustered together (Fig. 1B and C). The results of the pairwise permutational multivariate analysis of variance revealed differences in the microbial composition between C. parvum-infected and uninfected animals (p<0.05; Fig. 1D).

Assessing microbial abundance and association at different taxonomic levels

The taxonomic structure of the gut microbial composition in C. parvum-infected and uninfected goat kids was assessed. At the phylum level, Bacteroidetes and Firmicutes were predominant in both groups, followed by Proteobacteria and Actinobacteria (Fig. 2A). No significant difference in the Bacteroidetes/Firmicutes ratio was observed between the two groups (p>0.05; Fig. 3A).

Fig. 2. Taxonomic analysis of microbiota at the (A) phylum level and (B) class level between the two groups. The relative abundance of fecal bacteria in goat kids is shown.
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Fig. 3. The differences in relative abundance of selected taxa at (A) Bacteroidetes/Firmicutes ratio, (B) class Clostridia, and (C) class Bacilli.
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At the class level, Bacteroidia, Clostridia, Gammaproteobacteria, Bacilli, and Negativicutes were predominant (Fig. 2B). The relative abundances of Clostridia and Bacilli, known for their digestive roles in ruminants and belonging to the phylum Firmicutes, were compared; however, no significant differences were observed in either case (p>0.05; Fig. 3B and C).

At the species level, within the class Clostridia, Catabacter honkongensis, Coprococcus catus, Oribacterium parvum, Ruminococcus bromil, and Intestinibacter bartlettii were negatively associated with C. parvum infection, whereas Ruminococcus gnavus, Tyzzerella nexills, and Butyricicoccus pullicaecorum were positively associated (p<0.05; Fig. 4A). In addition, at the species level, within the class Bacilli, Faecalicoccus pleomorphus, Aerococcus vaginalis, and Streptococcus salivarius showed decreased relative abundance in the C. parvum-infected group (p<0.05; Fig. 4B).

Fig. 4. The differences in relative abundance of species within (A) class Clostridia and (B) class Bacilli. Only species showing statistically significant differences are shown (p<0.05).
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Differential abundance analysis was conducted to identify the significant differences in the abundance of taxa between the two groups. A volcano plot revealed elevated levels of Tyzzerella, Lactobacillus, Butyricicoccus, Enterococcus, and Negativicoccus whereas Aerococcus, Faecalicoccus, Oribacterium, and Coprococcus were less abundant in the C. parvum-infected group than in the uninfected group (Fig. 5A). At the species level, the heatmap indicated a notable increase in the abundance of T. nexillis, Lactobacillus johnsonii, B. pullicaecorum, Enterococcus raffinosus, Enterococcus faecalis, and Negativicoccus massiliensis, and a decreased abundance of A. vaginalis, F. pleomorphus, O. parvum, and Coprococcus comes (Fig. 5B).

Fig. 5. Differential abundance analysis of (A) principal coordinate analysis and (B) heatmap for the gut microbiome between Cryptosporidium parvum-infected and uninfected groups. The criteria for assessing significance were set at a fold change > 4, with corrected p<0.05.
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Several studies have reported alterations in the gut microbiota in response to Cryptosporidium infection in various animals [22-27]; however, there are few studies involving goats. In this study, the differences in microbial diversity between C. parvum-infected and uninfected goat kids were analyzed. Alpha diversity, which measures the number of species and their relative abundance, showed no significant differences except for the Shannon index. However, beta diversity, which assesses the differences in species composition between groups, indicated significant shifts in the microbial community composition due to C. parvum infection (p<0.05). This means that C. parvum-infected and uninfected goat kids harbored different specific species and their abundances. These findings demonstrate the impact of C. parvum infection on altering the gut microbial taxonomic composition and diversity.

A previous study showed that C. parvum infection dramatically alters gut microbial diversity in goat kids at 5 days post infection (dpi), whereas the microbial composition and diversity of the C. parvum-infected group are not significantly different from those of the control group at 15 dpi [28]. In the present study, PERMANOVA analysis showed a significant difference in microbial composition between the two groups (p<0.05), suggesting that the goats were in the early stages of C. parvum infection. PCoA is used to visualize the diversity and composition of microbial communities, where samples with similar microbial compositions clustered together on the graph. In this study, using the Bray-Curtis distance and Jaccard distance methods to represent dissimilarities, the C. parvum-infected group appeared distinct from the uninfected group, indicating the impact of this parasite on microbial communities in goat kids.

In the digestive system of ruminants, microbiota plays a crucial role in generating host enzymes, highlighting the importance of microbial diversity and abundance [14]. Firmicutes and Bacteroidetes are predominant in goat kids regardless of age or health status [9]. Firmicutes degrade fiber and cellulose in ruminants and produce short-chain fatty acids that regulate immune responses. Bacteroidetes are involved in the breakdown of carbohydrates and proteins and contribute to the development of the gastrointestinal immune system [14]. In a previous study, mice experimentally infected with C. parvum showed an elevated Bacteroidetes/Firmicutes ratio compared with the uninfected group [4]. Similar findings have been observed in pigs infected with Balantioides coli and mice infected with Giardia [17, 29], suggesting a common role for Bacteroidetes and Firmicutes in the gut microbiota. In this study, these two bacterial phyla were predominant in both groups, which is consistent with the results of previous studies; however, no significant difference in the ratio between these two groups was noted.

Analysis of microbiota diversity, conducted using a differential abundance test, revealed significant alterations in the microbial composition. Clostridia and Bacilli belonging to the phylum Firmicutes are involved in the digestive processes of ruminant animals. However, the abundance of Clostridia and Bacilli in C. parvum-infected goat kids was not significantly different from that in uninfected goat kids. As only a limited number of species within both classes exhibited significant alterations, further studies at the class level are required.

The genus Lactobacillus, which belongs to the class Bacilli, produces lactic acid [14]. Lactobacillus is often associated with healthy gut and is commonly used as an ingredient in probiotics. In this study, C. parvum-infected group showed statistically higher abundance of Lactobacillus which is different from our expectation. Previous studies on goat kids’ gut microbiome did not show a difference according to C. parvum infection [9, 28]. It is worth noting that a previous study suggested that C. parvum infection may be a cause of the development of secondary lactose intolerance [30]. Due to the limitation of the tested animal numbers in this study, we cannot conclude clear association between C. parvum infection and Lactobacillus, further studies are required.

In humans, Tyzzerella abundance is elevated in individuals with cardiovascular diseases. Furthermore, a pronounced increase in Tyzzerella is evident in individuals who follow unhealthy dietary patterns or are afflicted with Crohn’s disease. A previous study revealed that administering a probiotic supplement of bifidobacteria to mice resulted in a reduction in Tyzzerella levels [31]. In the present study, a significant increase in this genus was observed in the C. parvum-infected group, suggesting an association between Tyzzerella and C. parvum infection.

Enterococcus spp. are found in the intestinal flora of humans and E. faecalis is a common species known for its immunomodulatory role in both humans and animals [32]. Some species are used as probiotics; however, enterococci can also serve as pathogens. Previous studies have demonstrated the abundance of E. faecalis and E. raffinosus in patients with ulcerative colitis (UC) or inflammatory bowel disease (IBD) [33, 34]. The effects and pathogenesis of the increased presence of enterococci are not fully understood [35]; however, an association between these bacteria in the gut microbiota and UC or IBD has been observed [33, 34]. In the present study, the genus Enterococcus showed a significant increase in the group infected with C. parvum; this trend was also observed for E. faecalis and E. raffinosus. The precise effect of these bacteria remains unclear; nevertheless, they appear to be linked to alterations in the intestinal wall. Additionally, these bacteria notably exhibit antibiotic resistance, emphasizing the need for further research to better understand their roles and implications.

The gut microbiota is influenced by different internal and external factors such as age, diet, and antibiotic usage [7, 9]. The results of this study showed that infection with C. parvum and diarrhea affected the gut microbiota; however, some results were inconsistent with those of previous studies, such as the Bacteroidetes/Firmicutes ratio and microbial composition. As the goats included in this study were reared on a farm located in the environment, all samples were collected from a single farm to minimize external environmental factors. However, the farm differs from well-controlled experimental conditions, and various factors, including infection intensity (quantity of Cryptosporidium), period of diarrhea, dietary variations, and age, may influence the gut microbiota [14, 28].

This study examined the diversity and compositional changes in the gut microbiota of goat kids after C. parvum infection. The findings of this study showed that C. parvum infection, associated with diarrhea in neonatal goats, modulates the caprine intestinal microbiota. This research provides valuable insights into the interaction between C. parvum infection and the gut microbiota, thereby advancing our understanding of the pathogenesis of diarrhea associated with this parasite.

Conflict of Interest

No potential conflict of interest relevant to this article was reported.


This study was supported by the National Research Foundation of Korea (NRF) grant funded by the Korea government (MSIT) (No. 2021R1F1A1061795); the Korea Institute of Planning and Evaluation for Technology in Food, Agriculture, Forestry, and Fisheries (IPET) through the Agriculture, Food, and Rural Affairs Convergence Technologies Program for Educating Creative Global Leader, funded by the Ministry of Agriculture, Food, and Rural Affairs (MAFRA) (grant number: 320005-4).

Ethics Approval

The requirement for ethical review and approval was waived as this study focused on animal fecal samples. This study was conducted for diagnosis in goats. Animal contact during the examination was minimal, consistent with routine physical examination procedures, and was appropriately handled under the supervision of licensed veterinarians. None of the treatments were harmful or detrimental to animal welfare.



Laurent F, McCole D, Eckmann L, Kagnoff MF. Pathogenesis of Cryptosporidium parvum infection. Microbes Infect. 1999; 1:141-148


Klein P, Kleinová T, Volek Z, Šimůnek J. Effect of Cryptosporidium parvum infection on the absorptive capacity and paracellular permeability of the small intestine in neonatal calves. Vet Parasitol. 2008; 152:53-59


Deng M, Rutherford MS, Abrahamsen MS. Host intestinal epithelial response to Cryptosporidium parvum. Adv Drug Deliv Rev. 2004; 56:869-884


Mammeri M, Chevillot A, Thomas M, Julien C, Auclair E, Pollet T, Polack B, Vallée I, Adjou KT. Cryptosporidium parvum-infected neonatal mice show gut microbiota remodelling using high-throughput sequencing analysis: preliminary results. Acta Parasit. 2019; 64:268-275


Paul S, Sharma DK, Boral R, Mishra AK, Nayakwadi S, Banerjee PS, Pawaiya RS. Cryptosporidiosis in goats: a review. Adv Anim Vet Sci. 2014; 2:49-54


Zilber-Rosenberg I, Rosenberg E. Role of microorganisms in the evolution of animals and plants: the hologenome theory of evolution. FEMS Microbiol Rev. 2008; 32:723-735


Wang L, Xu Q, Kong F, Yang Y, Wu D, Mishra S, Li Y. Exploring the goat rumen microbiome from seven days to two years. PLOS ONE. 2016; 11e0154354


Li M, Zhou M, Adamowicz E, Basarab JA, Guan LL. Characterization of bovine ruminal epithelial bacterial communities using 16S rRNA sequencing, PCR-DGGE, and qRT-PCR analysis. Vet Microbiol. 2012; 155:72-80


Wang Y, Zhang H, Zhu L, Xu Y, Liu N, Sun X, Hu L, Huang H, Wei K, Zhu R. Dynamic distribution of gut microbiota in goats at different ages and health states. Front Microbiol. 2018; 9:2509


Han X, Yang Y, Yan H, Wang X, Qu L, Chen Y. Rumen bacterial diversity of 80 to 110-day-old goats using 16S rRNA sequencing. PLOS ONE. 2015; 10e0117811


Zhuang Y, Chai J, Cui K, Bi Y, Diao Q, Huang W, Usdrowski H, Zhang N. Longitudinal investigation of the gut microbiota in goat kids from birth to postweaning. Microorganisms. 2020; 8:1111


Liu F, Xie Y, Zajac AM, Hu Y, Aroian RV, Urban JF, Li RW. Gut microbial signatures associated with moxidectin treatment efficacy of Haemonchus contortus in infected goats. Vet Microbiol. 2020; 242:108607


Russell JB, Rychlik JL. Factors that alter rumen microbial ecology. Science. 2001; 292:1119-1122


Cholewińska P, Czyż K, Nowakowski P, Wyrostek A. The microbiome of the digestive system of ruminants: a review. Anim Health Res Rev. 2020; 21:3-14


O’Hara AM, Shanahan F. The gut flora as a forgotten organ. EMBO Rep. 2006; 7:688-693


Malmuthuge N, Guan LL. Gut microbiome and omics: a new definition to ruminant production and health. Anim Front. 2016; 6:8-12


He K, Yan W, Sun C, Liu J, Bai R, Wang T, Qian W. Alterations in the diversity and composition of gut microbiota in weaned piglets infected with Balantioides coli. Vet Parasitol. 2020; 288:109298


Kim AY, Alkathiri B, Lee S, Min KD, Kim S, Lee SM, Lee WK, Kwak D, Lee SH. Outbreak of severe diarrhea due to zoonotic Cryptosporidium parvum and C. xiaoi in goat kids in Chungcheongbuk-do, Korea. Parasitol Res. 2023; 122:2045-2054


Burrello C, Giuffrè MR, Macandog AD, Diaz-Basabe A, Cribiù FM, Lopez G, Borgo F, Nezi L, Caprioli F, Vecchi M, Facciotti F. Fecal microbiota transplantation controls murine chronic intestinal inflammation by modulating immune cell functions and gut microbiota composition. Cells. 2019; 8:517


Callahan BJ, McMurdie PJ, Rosen MJ, Han AW, Johnson AJA, Holmes SP. DADA2: high-resolution sample inference from Illumina amplicon data. Nat Methods. 2016; 13:581-583


McMurdie PJ, Holmes S. phyloseq: an R package for reproducible interactive analysis and graphics of microbiome census data. PLOS ONE. 2013; 8e61217


Ras R, Huynh K, Desoky E, Badawy A, Widmer G. Perturbation of the intestinal microbiota of mice infected with Cryptosporidium parvum. Int J Parasitol. 2015; 45:567-573


Charania R, Wade BE, McNair NN, Mead JR. Changes in the microbiome of Cryptosporidium-infected mice correlate to differences in susceptibility and infection levels. Microorganisms. 2020; 8:879


McKenney EA, Greene LK, Drea CM, Yoder AD. Down for the count: Cryptosporidium infection depletes the gut microbiome in Coquerel’s sifakas. Microb Ecol Health Dis. 2017; 28:1335165


Chen X, Zhao X, Zhao C, Ashfaq H, Fakhar-e-Alam Kulyar M, Bhutta ZA, Ali MM, Mansoor MK, Li K. Cryptosporidium infection induced the dropping of SCFAS and dysbiosis in intestinal microbiome of Tibetan pigs. Microb Pathog. 2023; 174:105922


Gamsjäger L, Cirone KM, Schluessel S, Campsall M, Herik A, Lahiri P, Young D, Dufour A, Sapountzis P, Otani S, Gomez DE, Claire Windeyer M, Cobo ER. Host innate immune responses and microbiome profile of neonatal calves challenged with Cryptosporidium parvum and the effect of bovine colostrum supplementation. Front Cell Infect Microbiol. 2023; 13:1165312


Dong H, Chen X, Zhao X, Zhao C, Mehmood K, Kulyar MFA, Bhutta ZA, Zeng J, Nawaz S, Wu Q, Li K. Intestine microbiota and SCFAs response in naturally Cryptosporidium-infected plateau yaks. Front Cell Infect Microbiol. 2023; 13:1105126


Mammeri M, Obregón DA, Chevillot A, Polack B, Julien C, Pollet T, Cabezas-Cruz A, Adjou KT. Cryptosporidium parvum infection depletes butyrate producer bacteria in goat kid microbiome. Front Microbiol. 2020; 11:548737


Barash NR, Maloney JG, Singer SM, Dawson SC. Giardia alters commensal microbial diversity throughout the murine gut. Infect Immun. 2017; 85e00948-16


Scott Weese J, Kenney DG, O’Connor A. Secondary lactose intolerance in a neonatal goat. J Am Vet Med Assoc. 2000; 217:372-375


Gryaznova M, Dvoretskaya Y, Burakova I, Syromyatnikov M, Popov E, Kokina A, Mikhaylov E, Popov V. Dynamics of changes in the gut microbiota of healthy mice fed with lactic acid bacteria and bifidobacteria. Microorganisms. 2022; 10:1020


Krawczyk B, Wityk P, Gałęcka M, Michalik M. The many faces of Enterococcus spp.: commensal, probiotic and opportunistic pathogen. Microorganisms. 2021; 9:1900


Růžičková M, Vítězová M, Kushkevych I. The characterization of Enterococcus genus: resistance mechanisms and inflammatory bowel disease. Open Med. 2020; 15:211-224


Zhou Y, Chen H, He H, Du Y, Hu J, Li Y, Li Y, Zhou Y, Wang H, Chen Y, Nie Y. Increased Enterococcus faecalis infection is associated with clinically active Crohn disease. Medicine. 2016; 95e5019


Zhao H, Peng Y, Cai X, Zhou Y, Zhou Y, Huang H, Xu L, Nie Y. Genome insights of Enterococcus raffinosus CX012922, isolated from the feces of a Crohn’s disease patient. Gut Pathog. 2021; 13:71