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Fig. 3 in The gastrointestinal nematodes of plains and Grevy's zebras: Phylogenetic relationships and host specificity

Fig. 3. Crossocephalus viviparus extracted from fresh zebra faeces were often infected with an apparent fungus. Hyphae emerging from the head (left, right) and from the tail (centre) of infected worms and stained with lactophenol blue (right). (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)

Fig. 2 in The gastrointestinal nematodes of plains and Grevy's zebras: Phylogenetic relationships and host specificity

Fig. 2. Nematode prevalence in plains vs. Grevy's zebras in (a) a bipartite graph, where edge widths indicate prevalence in each zebra species, and (b) a linear regression, shown in black with shading representing standard error and the one-to-one line indicated by the dashed red line. Only sequences comprising>1% of total reads were used and they were clustered into mOTUs by 98% similarity. Taxon labels followed by a letter signify species-level matches (>98% similarity) to reference worms identified only to genus (see SI2), while those followed by a number represent sequences that matched a reference only to the genus level (>95% similarity). Black boxes/points are taxa without a match of>95% to any identified sequences. (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 The gastrointestinal nematodes of plains and Grevy's zebras: Phylogenetic relationships and host specificity

Fig. 1. Phylogeny of all sequenced Strongylidae with species-level taxon assignments from GenBank and the present study, coloured by genus (the same colour code is used across all figures in this paper). Branch tips were pruned such that only one tip was kept of all immediate sister taxa with identical taxon assignments, and the number of samples merged in each tip is indicated in parentheses. Bootstrap percentages over 50% are displayed in bold to highlight nodes with high support. Branch lengths represent the number of base substitutions per site, estimated with the Tamura 3-parameter model assuming gamma-distributed substitution rate variation.

Fig. 5 in Host and geographic differences in prevalence and diversity of gastrointestinal helminths of foxes (Vulpes vulpes), coyotes (Canis latrans) and wolves (Canis lupus) in Quebec´, Canada

Fig. 5. On the left, whole mounted Cryptocotyle lingua adult trematode stained with borax carmine (credit: Brent Wagner). On the right, distribution of foxes (Vulpes vulpes) infected with C. lingua in the Subarctic (samples (n) collected along James Bay and the St Lawrence estuary) and Humid Continental climate collected during winter 2016–2017 by trappers from Qu´ebec, Canada. Arrows indicate major waterways.

Fig. 2. A in Host and geographic differences in prevalence and diversity of gastrointestinal helminths of foxes (Vulpes vulpes), coyotes (Canis latrans) and wolves (Canis lupus) in Quebec´, Canada

Fig. 2. A) Parasite genus richness in foxes (Vulpes vulpes, blue), coyotes (Canis latrans, orange), and wolves (Canis lupus, gray) from Qu´ebec, Canada, determined by gross examination and fecal flotation combined (N = 250). Fewer foxes were uninfected than coyotes (p = 0.006). More foxes were infected by two parasite genera than coyotes (p = 0.004). B) Parasite genus richness between Subarctic (yellow) and Humid Continental climate (green) in foxes from Qu´ebec, Canada, determined by gross examination and fecal flotation combined (N = 155). No significant difference in parasite genera was seen in foxes between Subarctic and Humid Continental climate regions. Parasites counted in both histograms were: diphyllobothriids (likely Dibothriocephalus spp.), Echinococcus spp., Taenia spp., Capillaria spp., Toxascaris sp., Toxocara sp., Trichuris sp., Uncinaria sp., Alaria sp., Cryptocotyle sp., and Metorchis sp. Parasites observed in both fecal and gross examination were only counted once. Bars represent 95% confidence intervals. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)

Fig. 6 in Host and geographic differences in prevalence and diversity of gastrointestinal helminths of foxes (Vulpes vulpes), coyotes (Canis latrans) and wolves (Canis lupus) in Quebec´, Canada

Fig. 6. Distribution of foxes (Vulpes vulpes), coyotes (Canis latrans), and wolves (Canis lupus) infected with Toxascaris leonina (left, N = 55) and Toxocara canis (right, N = 19) in the Subarctic and Humid Continental climate collected during winter 2016–2017 by hunters and trappers from Qu´ebec, Canada.

Fig. 1. K in Host and geographic differences in prevalence and diversity of gastrointestinal helminths of foxes (Vulpes vulpes), coyotes (Canis latrans) and wolves (Canis lupus) in Quebec´, Canada

Fig. 1. K¨oppen climate regions and sampling distribution of foxes (Vulpes vulpes, N = 176), coyotes (Canis latrans, N = 77), and wolves (Canis lupus, N = 23) collected during winter 2016–2017 by hunters and trappers from Qu´ebec, Canada. Arrows indicate major waterways.

Fig. 4 in Host and geographic differences in prevalence and diversity of gastrointestinal helminths of foxes (Vulpes vulpes), coyotes (Canis latrans) and wolves (Canis lupus) in Quebec´, Canada

Fig. 4. Mixed taeniid infections in the Humid Continental climate in coyotes (Canis latrans) and wolves (Canis lupus) from Qu´ebec, Canada, following molecular analyses. Abbreviations on x-axis: E. can, Echinococcus canadensis; T. hyd, Taenia hydatigena; T. twi, T. twitchelli; T. kra, T. krabbei; T. pis, T. pisiformis-"like"; T. cra, T. crassiceps.

Fig. 3 in Host and geographic differences in prevalence and diversity of gastrointestinal helminths of foxes (Vulpes vulpes), coyotes (Canis latrans) and wolves (Canis lupus) in Quebec´, Canada

Fig. 3. Neighbour-joining tree of Jukes-Cantor distances among sequences of CO1 (alignment 450 bp using all sites) from Alaria available on GenBank as of 7 July 2021. Data from Alaria americana, including data from the present study, indicated by darker shaded cluster and white font. Sequences from A. alata are HM022221-3, KF751233-4, KP123416-20, KP123422-5, KX962374, KX962392, KX962395, KX962397-8, KX962402, KX962406, KX962415, KX962421, KX962433, KX962437, KX962454-5, KX962471-2, KX962481, KX962491, KY012317, MT103215-31; from Alaria sp. in Argentina KF572949, MH892076, MT328804-6; from Alaria sp. in Wisconsin, USA KT223036; from A. americana MZ605217-33 (present study) and MH536507 (indicated with an asterisk).

Fig. 2 in An alien parasite affects local fauna-Confirmation of Sinergasilus major (Copepoda: Ergasilidae) switching hosts and infecting native Silurus glanis (Actinopterygii: Siluridae) in Hungary

Fig. 2. Evolutionary history of Sinergasilus based on Bayesian Inference (BI) analysis of 18S rDNA with Ergasilus anchoratus Markewitsch, 1940 designated as outgroup. Support for both maximum likelihood (ML, 1000 bootstrap replicates) and BI (10 million MCMC) indicated at nodes (ML/BI), only nodes with more than 50% support annotated.

Fig. 1 in An alien parasite affects local fauna-Confirmation of Sinergasilus major (Copepoda: Ergasilidae) switching hosts and infecting native Silurus glanis (Actinopterygii: Siluridae) in Hungary

Fig. 1. Micrographs using light microscopy (LM) and scanning electron microscopy (SEM) of Sinergasilus major; (A) Total body (SEM), (B) rostral plate with integumental pores and tactile setules (SEM), (C) thoracic plate with pectinate denticles (SEM), (D) ventral aspect of cephalon (SEM), (E) everted mouth (SEM), (F) inverted mouth (SEM), (G) ventral view of mouth parts (SEM), (H) mouth parts (LM). A1 – antennule 1, A2 – antenna, Ip – integumental pore, Gs – genital somite, Lb – labium, Lr – labrum, M – mouth, Md – mandible, Ml – maxillule, Mx – maxilla, Ps4 – pedigerous somite 4, Pd – pectinate denticles, Tp – thoracic plate, Ts – tactile setules.

Fig. 3 in First report of the nematode Cruzia tentaculata using molluscs as natural intermediate hosts, based on morphology and genetic markers

Fig. 3. Scanning Electron Microscope images of a Cruzia tentaculata larvae recovered from Achatina fulica: A) Anterior extremity and detail of the apical view showing the oral opening; B) Cephalic extremity with labial papillae and phasmids (arrows), apical view; C) Lateral view showing the lateral line (arrow); D) posterior region, lateral view showing the lateral line (arrow); E) posterior region, ventral view, and (e) detail of the anus.

Fig. 2 in First report of the nematode Cruzia tentaculata using molluscs as natural intermediate hosts, based on morphology and genetic markers

Fig. 2. Photomicrographs of the Cruzia tentaculata larvae recovered from A. fulica; A) Anterior extremity, showing the excretory pore (ep), bulb, and pre-bulbar dilatation; (a) details of the excretory pore in lateral view; B) Cephalic extremity showing the labial papillae and the teeth (t), apical view; b) Trilabial mouth, apical view; C) Pre-bulbar dilatation (pb) and well developed bulb; D) Lateral lines (arrows), transversal section; E) Posterior extremity, lateral view; (e) detail of the extremity of the tail; F) anus (a), with prominent opening lateral view and a pair of anal glands (arrow).

Fig. 1 in First report of the nematode Cruzia tentaculata using molluscs as natural intermediate hosts, based on morphology and genetic markers

Fig. 1. Line drawings of Cruzia tentaculata recovered from the molluscs in the present study, based on light microscopy. A) side view of the anterior region of a nematode recovered from Achatina fulica; B) side view of the posterior region of a nematode from A. fulica; C) Lateral view of a whole specimen recovered from Latipes erinaceus. Scale bar = 100 μm.

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Fig. 3 in Detection of Eumonospora henryae (Apicomplexa: Sarcocystidae) from Falco columbarius (Falconiformes: Aves): Comparison of host-parasite phylogram and comments on the family Sarcocystidae Poche, 1913

Fig. 3. Phylograms of the genus Eumonospora on the left and core land birds modified from McClure et al. (2019) on the right. The boxes under Eumonospora spp. represent detected host species and the shaded boxes encompass the Afroaves. The lines connect parasites and hosts encountered, with the dotted line indicating host switching across order boundaries.

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Fig. 1 in Detection of Eumonospora henryae (Apicomplexa: Sarcocystidae) from Falco columbarius (Falconiformes: Aves): Comparison of host-parasite phylogram and comments on the family Sarcocystidae Poche, 1913

Fig. 1. Optical (A, B) and differential interference contrast photomicrographs (C, D) of oocysts and sporocysts of Eumonospora sp. detected from Falco columbarius. Fig. 1A. Sporulated oocyst with stout sporozoites (SZ) inside a sporocyst (SP). Fig. 1B. A collapsed oocyst with a compact sporocyst residuum (SR) within an SP. Fig. 1C. Randomly diffused SR within an SP. Fig. 1D. Eight SZs with diffused SR. Scale bars = 10 μm.

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Fig. 2 in Detection of Eumonospora henryae (Apicomplexa: Sarcocystidae) from Falco columbarius (Falconiformes: Aves): Comparison of host-parasite phylogram and comments on the family Sarcocystidae Poche, 1913

Fig. 2. Phylogenetic trees based on three concatenated datasets (A: 18S + cox1, B: 18S + 28S, and C: 28S + cox1). Phylogenetic analyses are performed via Bayesian inference (BI) and maximum likelihood (ML) methods. Nodes are labelled with probability for BI method node support (left) and bootstrap value support for the ML method (right). Similar phylograms are illustrated with both methods in all datasets. Monophyletic clade of Eumonospora spp. branches off earlier than the clade of Besnoitia spp. and the clade comprising genera Hammondia, Heydornia, Neospora, and Toxoplasma. 18S: nuclear small subunit ribosomal DNA; 28S: nuclear large subunit ribosomal DNA; cox1: mitochondrial Cytochrome C oxidase subunit 1; NA: not available.

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Fig. 1 in Helminth's assemblage of a small frog in the Brazilian semiarid: parasite-host-environment relationships

Fig. 1. Parasite load (total number of helminths per host) between females (N= 41) and males (N= 53) of Pseudopaludicola pocoto (Anura) from AssÚ municipality, Rio Grande do Norte state, northeastern Brazil.

Fig. 1 in Helminth's assemblage of Trachemys dorbigni (Testudines: Emydidae) in southern Brazil: implications of anthropogenic environments and host's genders

Fig. 1. Overall layout of the collection environments in the study of helminth assemblage of Trachemys dorbigni in southern Brazil: A, detail of the Centro Agropecuário da Palma (UFPel), rural area of CapÃo do LeÃo, State of Rio Grande do Sul, Brazil; B, detail of the urban Área of Pelotas, Rio Grande do Sul, Brazil. Source: extracted and modified the site Google® Earth (©2014 Google – Images ©2014 Digital Globe).