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92 results for “helminth parasite”
A droplet digital polymerase chain reaction assay to detect rare helminth parasites infecting natural host populations (Vancouver Island 2023, University of Wisconsin Madison Laboratory colony 2024)
Helminth infections represent a significant challenge to human, livestock, and wildlife health, yet they remain relatively under-studied, especially in terms of their ecological impacts. Better understanding of how these parasites spread in wildlife populations could improve our ability to predict and manage disease transmission across various species. Traditional detection methods, such as visually identifying parasites in environmental samples or infected hosts, often fall short, especially during the early stages of infection when parasite loads are minimal. In this study, we introduce a highly sensitive and precise droplet digital PCR (ddPCR) assay that quantifies helminth DNA in aquatic habitats, focusing on the 18S rRNA gene as a marker. These data utilize the model host-parasite system between the tapeworm Schistocephalus solidus, and its cyclopoid copepod host, Acanthocyclops robustus. The molecular assays are built around creating an infection standard in the lab, where copepods were singly infected with a single tapeworm parasite. We extracted DNA from 100 infected adults and used this as a standard to translate gene copy numbers from the ddPCR reactions to actual animal values. After creating a known lab standard, we then use the generated probes and primers to detect (and quantify!) infection burdens in field samples, which include both water filter samples (eDNA) and zooplankton tows from several lakes around Vancouver Island, B.C. The data presented here include well-specific data from ddPCR runs (amplitude of individual level oil droplets in the reaction) as well as each ddPCR analysis in its entirety. In order to prove the specificity of probes and probe-primers, we include here ddPCR runs of closely related helminth species, Schistocephalus cotti and Schistocephalus pungitii. We also consider the binding to another genera of copepod, the calanoid Eurytomora. All of the data wrangling, analysis, and data visualization are included as .Rmd files in th
Fig. 1 in Review Of The Helminths Parasitic In Rare Aquatic Birds In Ukraine
Fig. 1. Localities of the material collection: — based on collection and literature; — based on collection; — based on literature.
Fig. 2 in Helminths Of Antarctic Rockcod Notothenia Coriiceps (Perciformes, Nototheniidae) From The Akademik Vernadsky Station Area (Argentine Islands, West Antarctica): New Data On The Parasite Community
Fig. 2. Average number of cysts of Corynosoma spp. in the body cavity of Notothenia coriiceps of five size groups.
Fig. 1 in Helminths Of Antarctic Rockcod Notothenia Coriiceps (Perciformes, Nototheniidae) From The Akademik Vernadsky Station Area (Argentine Islands, West Antarctica): New Data On The Parasite Community
Fig. 1. Prevalence (in %) and mean intensity of helminth species found in Notothenia coriiceps in the waters surrounding the Ukrainian Antarctic station "Akademik Vernadsky" in 2014–2015.
Figure 2. Dendrogram resulting from a in Host specificity and the structure of helminth parasite communities of fishes in a Neotropical river in Mexico
Figure 2. Dendrogram resulting from a similarity matrix based on the Sørensen measure for component communities of adult autogenic helminth parasites of 10 fish species from Apazapan, Río La Antigua, Veracruz, Mexico. Host species are: Amex, A. mexicanus; Rgua, R. guatemalensis; Smar, S. marmoratus; Hbim, P. bimaculata; Pmex, Poecilia mexicana; Pgra, Poeciliosis gracilis; Psph, Poecilia sphenops; Xell, X. helleri; Tell, T. ellioti; Vfen, V. fenestrata.
Figure 1 in Host specificity and the structure of helminth parasite communities of fishes in a Neotropical river in Mexico
Figure 1. Patterns of relative abundance of 24 species of helminths in 11 component communities of freshwater fishes from Río Apazapan, Río La Antigua basin, Mexico (fish species: Am, A. mexicanus; Rg, Rhamdia guatemalensis; Hb, Pseudoxiphophorus bimaculata; Pm, Poecilia mexicana; Ps, P. sphenops; Pg, Poeciliopsis gracilis; Xh, Xiphophorus helleri; Te, Thorichthys helleri; Vf, Vieja fenestrata; Sm, Sicydium gymnogaster).
Fig. 1. 2D in Proteomic profile of Ortleppascaris sp.: A helminth parasite of Rhinella marina in the Amazonian region
Fig. 1. 2D gel containing the somatic extract of Ortleppascaris sp. larvae. See Table 1 for details.
Fig. 1 in Reduced helminth parasitism in the introduced bank vole (Myodes glareolus): More parasites lost than gained
Fig. 1. Frequency distribution of intestinal helminth species richness in wood mice and bank voles examined in 2011 and 2012.
Fig. 5 in Helminth parasites of howler and spider monkeys in Mexico: Insights into molecular diagnostic methods and their importance for zoonotic diseases and host conservation
Fig. 5. Phylogenetic trees based on 28S (left) and cox1 (right) sequences of Strongyloides eggs. Sequences obtained from the eggs are bold type and indicated with an *. Numbers at the nodes represent posterior probabilities from Bayesian inference.
Fig. 2 in Helminth parasites of howler and spider monkeys in Mexico: Insights into molecular diagnostic methods and their importance for zoonotic diseases and host conservation
Fig. 2. Egg morphotypes found in the faeces of Mexican primates. A) Trypanoxyuris sp., B) Controrchis biliophilus, arrow pointing to the two eyespot remnants; C) trematode, diagnosed as C. biliophilus by molecular data; D) unidentified ancylostomatid; E) Strongyloides sp.; F) unidentified ascarid. Scale bar is equal to 15 Mm.
Fig. 4 in Helminth parasites of howler and spider monkeys in Mexico: Insights into molecular diagnostic methods and their importance for zoonotic diseases and host conservation
Fig. 4. Phylogenetic tree based on 28S sequences of Controrchis biliophilus. Sequences obtained from the eggs are bold type and indicated with an *. Numbers at the nodes represent posterior probabilities from Bayesian inference. Host species are indicated within parenthesis.
Fig. 1 in Helminth parasites of howler and spider monkeys in Mexico: Insights into molecular diagnostic methods and their importance for zoonotic diseases and host conservation
Fig. 1. Surveyed sites for parasites in Mexican primates. Dots indicate sampling sites, black: Alouatta palliata; white: A. pigra; and grey: Atetes geoffroyi. Polygons indicate the primate distribution range in Mexico, diagonal lines: A. palliata; dashes: A. pigra; and grey: A. geoffroyi.
Fig. 3 in Helminth parasites of howler and spider monkeys in Mexico: Insights into molecular diagnostic methods and their importance for zoonotic diseases and host conservation
Fig. 3. Phylogenetic trees based on 28S (left) and cox1 (right) sequences of Trypanoxyuris sp. Sequences obtained from the eggs are bold type and indicated with an *. Numbers at the nodes represent posterior probabilities from Bayesian inference.
Fig. 1 in Helminths in common eiders (Somateria mollissima): Sex, age, and migration have differential effects on parasite loads
Fig. 1. Distributions of breeding and wintering populations of S. m. borealis, S. m. dresseri, and S. m. sedentaria in North America and Greenland. Populations of S. m. borealis are wintering in two areas in the pictured region; one in Southwest Greenland and one in East Canada (Newfoundland and Labrador). Individuals wintering in Southwest Greenland migrate to breed in West Greenland or Arctic Canada, whereas individuals wintering in East Canada have breeding areas in Arctic Canada (illustrated by the different direction of the red diagonal lines). For S. m. dresseri the breeding and wintering ranges overlap in one area that covers Newfoundland and Labrador as well as the northeastern part of the US, as shown by the grey horizontal lines. The subspecies S. m. sedentaria has its year-round residence in the Hudson Bay area as shown by the blue vertical lines. Dark stars mark the sampling locations of eiders in this study, whereas the white star marks the sampling location of eiders by Tourangeau et al. (2018). (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 Helminths in common eiders (Somateria mollissima): Sex, age, and migration have differential effects on parasite loads
Fig. 3. Prevalences of the cestodes Lateriporus sp. (A) and Microsomacanthus spp. (B), and the acanthocephalan Profilicollis sp. (C) in common eiders. Abbreviations: bor, CD = S. m. borealis, Cape Dorset; bor, GRLD = S. m. borealis, Greenland; bor, NFLD = S. m. borealis, Newfoundland; dre, NFLD = S. m. dresseri, Newfoundland; sed, BI = S. m. sedentaria [data published in Tourangeau et al. (2018)]. n-m = non-migratory, po-m = post-migratory, prm = pre-migratory. Letters describe significant differences between groups: if two groups share a letter, there is no significant difference in their prevalences.
Fig. 2 in Helminths in common eiders (Somateria mollissima): Sex, age, and migration have differential effects on parasite loads
Fig. 2. Examples of gastrointestinal parasites retrieved from common eiders in this study. (A) The trematode Notocotylus sp., (B) the cestode Lateriporus sp., (C) the acanthocephalan, Profilicollis sp. (D) microphallid trematodes, and (E) Microsomacanthus spp. cestodes.
Fig. 5 in Helminths in common eiders (Somateria mollissima): Sex, age, and migration have differential effects on parasite loads
Fig. 5. Cumulative percentages of birds infected with (A) Microsomacanthus spp., (B) Microphallus spp. and (C) Gymnophallus spp. from five different locations. Legend denotes the five infection levels: 0, 1s, 10s, 100s, and 1000s of parasite individuals within a single host. Abbreviations: bor, GRLD = S. m. borealis, Greenland; bor, NFLD = S. m. borealis, Newfoundland; dre, NFLD = S. m. dresseri, Newfoundland; bor, CD = S. m. borealis, Cape Dorset; sed, BI = S. m. sedentaria, Belcher Islands [data published in (Tourangeau et al., 2018)]. nm = non-migratory, po-m = post-migratory, pr-m = pre-migratory.
Figure 1 in Detection of helminth parasites in commercialized turtles: threats to native Testudines in northeast India
Figure 1. Astiotrema reniferum: (A) entire, ventral view (arrow marks anterior to posterior denoted ovary, anterior testis, and posterior testes), (B) Anterior end, ventral view (arrow marks anterior to posterior denoted oral sucker, gonopore, acetabulum, and ovary), (C) Gonopore, and egg are marked by arrow anterior to posterior, and (D) Testes, ventral view.
Fig. 1 in Diversity of helminth parasites of eight siluriform fishes from the Aguapeí River, upper Paraná basin, São Paulo state, Brazil
Fig. 1. Map of the study area. Black dots represent the sampling location in the mouth of the Aguapeí River, Upper Paraná River basin, at the border of São Paulo and Mato Grosso do Sul States, Brazil.
Fig. 1 in Diversity of helminth parasites of freshwater fish in the headwaters of the Coatzacoalcos River, in Oaxaca, Mexico
Fig. 1. The upper Coatzacoalcos river in Mexico showing the fish Collection sites; codes: 1. El Platanillo river, tributary to Del Sol river (municipality Santo Domingo Petapa), coordinates 16.951111, −95.244167, altitude 416 m; 2. Río Grande (El Barrio), 16.792167, −95.016083, 220 m; 3. Río Negro (Santa María Chimalapa), 16.898528, −94.693694, 166 m; 4. Río Modelo (Santa María Chimalapa), 17.134778, −94.745000, 115 m; 5. Río Pánfilo (Matías Romero, Oaxaca), 17.083639, −94.873944, 60 m; 6. Río Jaltepec (Jesús Carranza, Veracruz), 17.388444, −95.056111, 40 m; 7. Río Escondido (Paraje San Francisco El Vado, Agencia Municipal Río Escondido, Santa María Chimalapa), 17.091083, −94.751694, 103 m. Note all sites in Oaxaca state, except # 6.
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