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66 results for “gastrointestinal parasite”
Fig. 1 in Veterinary monitoring of gastrointestinal parasites in European bison, Bison bonasus designated for translocation: Comparison of two coprological methods
Fig. 1. Probability of detection of Eimeria spp. oocysts with the modified McMaster technique based on the number of oocysts detected using the Willis technique.
Fig. 4 in Veterinary monitoring of gastrointestinal parasites in European bison, Bison bonasus designated for translocation: Comparison of two coprological methods
Fig. 4. The relationship between the prevalence of various taxa eggs/oocysts in European bison feces measured by the Willis and modified McMaster techniques (each point represents an individual taxon/genus, blue points stand for oocysts and red point for eggs). (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)
Fig. 3 in Veterinary monitoring of gastrointestinal parasites in European bison, Bison bonasus designated for translocation: Comparison of two coprological methods
Fig. 3. Probability of detection of Trichostrongylidae eggs with the modified McMaster technique based on the number of eggs detected using the Willis technique.
Fig. 4 in Effect of urbanization on zoonotic gastrointestinal parasite prevalence in endemic toque macaque (Macaca sinica) from different climatic zones in Sri Lanka
Fig. 4. Number of parasite genera types (species richness) infecting M. s. aurifrons, M. s. sinica and M. s. opisthomelas in urban, suburban, and wild habitats.
Fig. 2 in Veterinary monitoring of gastrointestinal parasites in European bison, Bison bonasus designated for translocation: Comparison of two coprological methods
Fig. 2. Probability of detection of Trichuris sp. eggs with the modified McMaster technique based on the number of eggs detected using the Willis technique.
Fig. 1 in Effect of urbanization on zoonotic gastrointestinal parasite prevalence in endemic toque macaque (Macaca sinica) from different climatic zones in Sri Lanka
Fig. 1. The three subspecies of macaque's endemic to Sri Lanka. (A) Common macaque (Macaca sinica sinica), (B) dusky or pale-fronted macaque (M. s. aurifrons), and (C) hill-zone macaque (M. s. opisthomelas) (image courtesy: Madura De Silva).
Fig. 2 in Demographic, environmental and physiological predictors of gastrointestinal parasites in urban raccoons
Fig. 2. Nematode and coccidia faecal egg/oocyst counts in raccoons are associated with raccoon age and the month (season) of sampling. (A) Baylisascaris nematodes; (B) strongyle type nematodes; (C) capillariid type nematodes; (D) coccidia.
Fig. 1 in Demographic, environmental and physiological predictors of gastrointestinal parasites in urban raccoons
Fig. 1. Photographs of nematode eggs and oocysts taken at 40× magnification. (A) Ascarid type nematodes (likely Baylisascaris procyonis); (B) strongyle type nematodes (Placoconis lotoris or Molineus barbatus); (C) capillariid type nematodes (Capillaria procyonis or Capillaria putorii); (D) "large" oocysts; (E) "small" oocysts; (F) "long" oocysts. Scale bar = 20 μm in all photographs.
Fig. 4 in Demographic, environmental and physiological predictors of gastrointestinal parasites in urban raccoons
Fig. 4. Distribution of coinfections in juvenile raccoons sampled in October and yearling raccoons sampled in July. Raccoons could be infected by 0–4 types of parasite. There was no significant difference between cross-sectionally (A) and longitudinally (B) sampled raccoons in the mean number of types of parasite harboured as juveniles in October, suggesting that parasite coinfections do not contribute to overwinter mortality. However, raccoons tended to clear parasite infections rather than gain them during this interval (C).
Fig. 3 in Demographic, environmental and physiological predictors of gastrointestinal parasites in urban raccoons
Fig. 3. Changes in gastrointestinal nematode and coccidia infection status and faecal egg or oocyst count for raccoons that were sampled in both July and October of the same year, stratified by age class. (A) Baylisascaris nematodes; (B) strongyle type nematodes; (C) capillariid type nematodes; (D) coccidia. Juvenile raccoons tended to gain nematode infections between July and October. Both adult and juvenile raccoons that were infected with coccidia in July tended to remain infected when resampled in October. Change in egg count = October egg count – July egg count. On average, the faecal egg count of juvenile raccoons increased more than the adult faecal egg count for Baylisascaris, strongyle, and capillariid nematodes (Welch's two sample t-test; pvalue <0.05), but there was no difference in the change in oocyst count for adults vs juveniles.
Fig. 2 in Patterns of gastrointestinal parasite infections in bighorn sheep, Ovis canadensis, with respect to host sex and seasonality
Fig. 2. Seasonal differences in fecal egg counts in female (blue) and male (red) bighorn sheep. Point intervals display the mean count ±95% confidence intervals as predicted by generalised linear mixed effects models. Seasons are: Late gestation (Late gestation/early lactation between April to June); Lactation/summer (between July and October); Rut (November and December); Winter (Winter/early gestation from January to March). Parasites are a) Strongyle; b) Nematodirus; c) Marshallagia; d) Protostrongylus lungworm; e) Eimeria. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)
Fig. 1 in Patterns of gastrointestinal parasite infections in bighorn sheep, Ovis canadensis, with respect to host sex and seasonality
Fig. 1. Schematic of the reproductive biology and seasons of bighorn sheep. The blue circle represents the entire year, where the top is December, 3 o'clock March, 6 o'clock June, 10 o'clock October etc. The grey quarter circle represents the season Jan–March = Winter/early gestation; the dark green quarter circles represent the season from April–June = late gestation/early lactation; the light green line represents the season between July and October, which is also representing lactation/summer; and the brown line is representing November and December, or the rutting season. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)
Fig. 3 in Patterns of gastrointestinal parasite infections in bighorn sheep, Ovis canadensis, with respect to host sex and seasonality
Fig. 3. Differences in mean and standard error in strongyle counts between males that use the coursing or tending mating tactic. Point intervals display the mean count ±95% confidence intervals as predicted by the generalised linear mixed effects model.
Experimental parasite community perturbation reveals associations between Sin Nombre virus and gastrointestinal nematodes in a rodent reservoir host
<p>Individuals are often co-infected with several parasite species, yet measuring within-host interactions remains difficult in the wild. Consequently, the impact of such interactions on host fitness and epidemiology are often unknown. We used anthelmintic drugs to experimentally reduce nematode infection and measured the effects on both nematodes and the important zoonosis Sin Nombre virus (SNV) in its primary reservoir (<i>Peromyscus spp.</i>). Treatment significantly reduced nematode infection, but increased SNV seroprevalence. Furthermore, mice that were co-infected with both nematodes and SNV were in better condition and survived up to four times longer than uninfected or singly-infected mice. These results highlight the importance of investigating multiple parasites for understanding interindividual variation and epidemiological dynamics in reservoir populations with zoonotic transmission potential.</p>
Fig. 4 in Gastrointestinal parasites in captive and free-ranging Cebus albifrons in the Western Amazon, Ecuador
Fig. 4. Cumulative egg and cyst count of parasites from each sample.
Fig. 2 in Gastrointestinal parasites in captive and free-ranging Cebus albifrons in the Western Amazon, Ecuador
Fig. 2. Cumulative richness from the first sample to the third sample for the 26 animals sampled.
Fig. 3 in Gastrointestinal parasites in captive and free-ranging Cebus albifrons in the Western Amazon, Ecuador
Fig. 3. Cumulative prevalence of parasites from each sample.
Fig. 1 in Gray wolves as sentinels for the presence of Echinococcus spp. and other gastrointestinal parasites in France
Fig. 1. Distribution of wolf fecal samples analyzed according to season and year.
Fig. 1 in Gastrointestinal parasite diversity of South American camelids (Artiodactyla: Camelidae): First review throughout the native range of distribution
Fig. 1. PRISMA flowchart of the systematic review process.
Experimental parasite community perturbation reveals associations between Sin Nombre virus and gastrointestinal nematodes in a rodent reservoir host
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