Abstract:The whipworms, i.e. parasitic nematodes of the genus Trichuris Roederer, 1761, infect a variety of mammals. Apparently low diversity of primate-infecting species of Trichuris strongly contrasts with the high number of species described in other mammalian hosts. The present study addresses the diversity of whipworms in captive and free-ranging primates and humans by analysing nuclear (18S rRNA, ITS2) and mitochondrial (cox1) DNA. Phylogenetic analyses revealed that primate whipworms form two independent lineages: (i) the Trichuris trichiura (Linnaeus, 1771) clade comprised of genetically almost identical whipworms from human and other primates, which suggests the ability of T. trichiura to infect a broader range of primates; (ii) a clade containing primarily Trichuris suis Schrank, 1788, where isolates from human and various primates formed a sister group to isolates from pigs; the former isolates thus may represent of more species of Trichuris in primates including humans. The analysis of cox1 has shown the polyphyly of the genera Trichuris and Capillaria, Zeder, 1800. High sequence similarity of the T. trichiura isolates from humans and other primates suggests their zoonotic potential, although the extent of transmission between human and other non-human primates remains questionable and requires further study.

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Bifidobacteria, which commonly inhabit the primate gut, are beneficial contributors to host wellbeing. Anatomical differences and natural habitat allow an arrangement of primates into two main parvorders; New World monkeys (NWM) and Old World monkeys (OWM). The number of newly described bifidobacterial species is clearly elevated in NWM. This corresponds to our finding that bifidobacteria were the dominant group of cultivated gut anaerobes in NWM, while their numbers halved in OWM and were often replaced by Clostridiaceae with sarcina morphology. We examined an extended MALDI-TOF MS database as a potential identification tool for rapid screening of bifidobacterial distribution in captive primates. Bifidobacterial isolates of NWM were assigned mainly to species of primate origin, while OWM possessed typically multi-host bifidobacteria. Moreover, bifidobacterial counts reflected the feed specialization of captive primates decreasing from frugivore-insectivores, gummivore-insectivores, frugivore-folivores to frugivore-omnivores. Amplicon sequencing analysis supported this trend with regards to the inverse ratio of Actinobacteria and Firmicutes. In addition, a significantly higher diversity of the bacterial population in OWM was found. The evolution specialization of primates seems to be responsible for Bifidobacterium abundance and species occurrence. Balanced microbiota of captive primates could be supported by optimized prebiotic and probiotic stimulation based on the primate host.

Infections caused by the intestinal ciliate Neobalantidium coli are asymptomatic in most hosts. In humans and captive African great apes clinical infections occasionally occur, manifested mainly by dysentery; however, factors responsible for development of clinical balantidiasis have not been fully clarified. We studied the effect of dietary starch on the intensities of infection by N. coli in two groups of captive chimpanzees. Adult chimpanzees infected by N. coli from the Hodonín Zoo and from the Brno Zoo, Czech Republic, were fed with a high starch diet (HSD) (average 14.7% of starch) for 14 days, followed by a five-day transition period and subsequently with a period of low starch diet (LoSD) (average 0.1% of starch) for another 14 days. We collected fecal samples during the last seven days of HSD and LoSD and fixed them in 10% formalin. We quantified trophozoites of N. coli using the FLOTAC method. The numbers of N. coli trophozoites were higher during the HSD (mean ± SD: 49.0±134.7) than during the LoSD (3.5±6.8). A generalized linear mixed-effects model revealed significantly lower numbers of the N. coli trophozoites in the feces during the LoSD period in comparison to the HSD period (treatment contrast LoSD vs. HSD: 2.7±0.06 (SE), z = 47.7; p<<0.001). We conclude that our data provide a first indication that starch-rich diet might be responsible for high intensities of infection of N. coli in captive individuals and might predispose them for clinically manifested balantidiasis. We discuss the potential nutritional modifications to host diets that can be implemented in part to control N. coli infections.

Five Bifidobacterium strains, VB23T, VB24T, VB25T, VB26T and VB31T, were isolated from chimpanzee (Pan troglodytes), cotton-top tamarin (Saguinus oedipus), Goeldi’s marmoset (Callimico goeldii), moustached tamarin (Saguinus mystax) and patas monkey (Erythrocebus patas), respectively, which were kept in two Czech zoos. These strains were isolated from faecal samples and were Gram-positive, non-motile, non-sporulating, anaerobic and fructose-6-phosphate phosphoketolase-positive. Phylogenetic analyses based on 16S rRNA revealed close relatedness between VB23T and Bifidobacterium angulatum LMG 11039T (96.0 %), VB24T and Bifidobacterium pullorum subsp. pullorum DSM 20433T (96.1 %), VB25T and Bifidobacterium goeldii LMG 30939T (96.5 %), VB26T and Bifidobacterium imperatoris LMG 30297T (98.1 %), and VB31T and B . angulatum LMG 11039T (99.40 %). Internal transcribed spacer profiling revealed that VB23T, VB24T, VB25T, VB26T and VB31T had highest similarity to Bifidobacterium breve LMG 13208T (77.2 %), Bifidobacterium longum subsp. infantis ATCC 15697T (85.8 %), Bifidobacterium biavatii DSM 23969T (76.9 %), B. breve LMG 13208T (81.2 %) and B. angulatum LMG 11039T (88.2 %), respectively. Average nucleotide identity (ANI) and digital DNA–DNA hybridization (dDDH) analyses with their closest neighbours supported the independent phylogenetic positions of the strains with values between 86.3 and 94.3 % for ANI and 25.8 and 54.9 % for dDDH. These genomic and phylogenetic analyses suggested that the evaluated strains were novel Bifidobacterium species named Bifidobacterium erythrocebi sp. nov. (VB31T=DSM 109960T=CCUG 73843T), Bifidobacterium moraviense sp. nov. (VB25T=DSM 109958T=CCUG 73842T), Bifidobacterium oedipodis sp. nov. (VB24T=DSM 109957T=CCUG 73932T), Bifidobacterium olomucense sp. nov. (VB26T=DSM 109959T=CCUG 73845T) and Bifidobacterium panos sp. nov. (VB23T=DSM 109963T=CCUG 73840T).