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Fig. 1 in Prevalence and molecular characterisation of Acanthocephala in pinnipedia of the North and Baltic Seas

Fig. 1. Prevalence of acanthocephalan infections in harbour and grey seals from the German North and Baltic Seas between 1996 and 2012. Notations indicate the Acanthocephala positive and total number of examined Phoca vitulina (Pv) and Halichoerus grypus (Hg). Connecting lines indicate statistically significant differences between annual prevalences after Holm–Bonferroni correction (P ≤ 0.001).

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Fig. 3 in Prevalence and molecular characterisation of Acanthocephala in pinnipedia of the North and Baltic Seas

Fig. 3. Phylogenetic analysis of the ribosomal ITS1-5.8S-ITS2-complex using the Maximum Likelihood method based on the Kimura 2-parameter model. The log likelihood is −16,028.00. The percentage of trees based on 1000 bootstrap replicates in which the associated taxa clustered together is shown next to the branches. GenBank accession numbers of analysed nucleotide sequences are listed in Table 1.

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Fig. 4 in The neglected diversity: Description and molecular characterisation of Trypanosoma haploblephari Yeld and Smit, 2006 from endemic catsharks (Scyliorhinidae) in South Africa, the first trypanosome sequence data from sharks globally

Fig. 4. Bayesian Inference (BI)/Maximum Likelihood (ML) analysis showing the phylogenetic position of Trypanosoma haploblephari (Yeld and Smit, 2006) genotypes representing morphotypes A and B inferred from partial 18S rRNA gene sequences. Comparative sequences representing known Trypanosoma species, with Trypanosoma avium (KT728402) as outgroup, were obtained from GenBank. Tree topologies for both the BI and ML trees were identical; the nodal support values (BI/ML) are represented on the BI tree. Some branches have been shortened with each //= 0.04 substitutions per site.

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Fig. 3 in The neglected diversity: Description and molecular characterisation of Trypanosoma haploblephari Yeld and Smit, 2006 from endemic catsharks (Scyliorhinidae) in South Africa, the first trypanosome sequence data from sharks globally

Fig. 3. Micrographs of Trypanosoma haploblephari (Yeld and Smit, 2006) morphotype A (A–C) and T. haploblephari morphotype B (D–F) in Giemsa-stained blood films of Haploblepharus pictus and Poroderma pantherinum, respectively. Blood stage with kinetoplast (k) and undulating membrane (μm) visible (A–C); slender forms (B, E); presence of a flagellum (f) in deeply stained individuals (C, F). Scale bar: 10 μm.

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Fig. 2 in The neglected diversity: Description and molecular characterisation of Trypanosoma haploblephari Yeld and Smit, 2006 from endemic catsharks (Scyliorhinidae) in South Africa, the first trypanosome sequence data from sharks globally

Fig. 2. Line drawing of Trypanosoma haploblephari (Yeld and Smit, 2006) from the host Poroderma pantherinum (Slide HE18-18) next to a drawing of a red blood cell.

Fig. 5 in Molecular characterisation of the Monogenea parasites of blue mackerel Scomber australasicus (Perciformes: Scombridae) in Australian waters

Fig. 5. Allogastrocotyle bivaginalis ex Scomber australasicus. a) Whole body; b) Oral suckers with pharynx; c) Copulatory organ; d) A typical clamp; e) Large anchors; f) Small anchors.

Fig. 1 in Molecular characterisation of the Monogenea parasites of blue mackerel Scomber australasicus (Perciformes: Scombridae) in Australian waters

Fig. 1. Kuhnia scombri ex Scomber australasicus. a) Whole body; b) Oral suckers with pharynx; c) Copulatory organ; d) A typical egg; e) A typical clamp; f) Large anchors; g) Small anchors.

Fig. 4 in Molecular characterisation of the Monogenea parasites of blue mackerel Scomber australasicus (Perciformes: Scombridae) in Australian waters

Fig. 4. Gastrocotyle kurra ex Scomber australasicus. a) Whole body; b) Oral suckers with pharynx; c) Copulatory organ; d) A typical egg; e) A typical clamp; f) Terminal lappet with anchors.

Fig. 3 in Molecular characterisation of the Monogenea parasites of blue mackerel Scomber australasicus (Perciformes: Scombridae) in Australian waters

Fig. 3. Pseudokuhnia minor ex Scomber australasicus. a) Whole body; b) Oral suckers with pharynx; c) Copulatory organ; d) A typical egg; e) A typical clamp; f) Large anchors.

Fig. 2 in Molecular characterisation of the Monogenea parasites of blue mackerel Scomber australasicus (Perciformes: Scombridae) in Australian waters

Fig. 2. Kuhnia scombercolias ex Scomber australasicus. a) Whole body; b) Copulatory organ; c) A typical egg; d) A typical clamp; e) Large anchors; f) Small anchors.

Fig. 6 in Molecular characterisation of the Monogenea parasites of blue mackerel Scomber australasicus (Perciformes: Scombridae) in Australian waters

Fig. 6. The Phylogenetic relationship of Monogenea identified from blue mackerel Scomber australasicus in this study compared with closely related species cox1 sequences available in GenBank (Table 2 for details). The tree has been constructed/inferred using the Bayesian method. *indicates the cox1 sequences generated in the present study. The Bayesian posterior probability values more than 95% were shown on the node.

Fig. 1. Myxobolus tihanyensis n in Morphological and molecular characterisation of two closely related species: Myxobolus tihanyensis n. sp. and Myxobolus sandrae Reuss, 1906

Fig. 1. Myxobolus tihanyensis n. sp. plasmodia inhabiting Perca fluviatilis. (A). Plasmodia in the mesenchymal tissue between the caudal fin rays beneath the skin. (B) Plasmodia in the subcutaneous muscle close to the cartilage and ossified caudal fin rays (C) Plasmodia close to the pleural centrum (pc) located in the homocercal caudal fin. (D) Plasmodia is shown in the homocercal caudal skeleton in the urostyle (u) and the hypural (h). Note plasmodia are indicated in black arrows. Scale bars = 500 μm.

Fig. 4 in Morphological and molecular characterisation of two closely related species: Myxobolus tihanyensis n. sp. and Myxobolus sandrae Reuss, 1906

Fig. 4. Histology sections of Perca fluviatilis using the haematoxylin and eosin (H & E) technique. (A–B) Sagittal section of the proximal region of the caudal fin. (A) Rounded plasmodia (p) developing in the mesenchyme (mh) closely attached to the bases of the rays (r), scale bar = 100 μm. (B) Higher magnification of plasmodiacontaining spores. Scale bar = 20 μm. (C–D) Transversal section of the caudal vertebrate region. (C) Plasmodia located between the hemal spine (hs) and muscular fibres (mf), scale bar = 200 μm. (D) Higher magnification of plasmodia containing spores (black arrows), scale bar = 20 μm.

Fig. 3 in Morphological and molecular characterisation of two closely related species: Myxobolus tihanyensis n. sp. and Myxobolus sandrae Reuss, 1906

Fig. 3. Schematic drawings of the mature spore of Myxobolus tihanyensis n. sp. from the caudal fin of Perca fluviatilis (A) in frontal view, (B) in sutural view. Scale bar = 10 μm.

Fig. 2 in Morphological and molecular characterisation of two closely related species: Myxobolus tihanyensis n. sp. and Myxobolus sandrae Reuss, 1906

Fig. 2. Photomicrographs of Myxobolus tihanyensis n. sp. spores from Perca fluviatilis. (A–D) Myxobolus tihanyensis n. sp., and (E–H), Myxobolus sandrae from Sander lucioperca. (A, E) Numerous mature spores (s) illustrate an ovoid shape and two polar capsules (pc). (B, F) Ovoid spores with sutural markings (white arrows) with two polar capsules which contain coiled polar tubules (pf) (C, G) Spore in sutural view showing the suture (su) (D, H) Spores releasing the polar tubules (pf) and showing sutural markings. Figs. C, G and H represented spores stained with Lugol solution. Scale bars = 10 μm.

Fig. 4 in Prevalence, molecular characterisation and phylogenetic analyses of hydatid cysts and cysticercus tenuicollis isolates and first report of E. canadensis (G6/G7) in wild boars in Bingol province, Türkiye

Fig. 4. Haplotype network of G1/G3 haplotypes identified on the basis of partial nad5 gene (628 bp). The G1 isolates obtained in this study (Hap01-Hap04), G3 isolates (Hap05, Hap06). Hatch marks represent the number of mutations between the haplotypes and the size of circle corresponds to the frequency of each haplotype in the population. Haplotypes formed by the isolates obtained in this study are marked with an asterisk.

Fig. 3. Haplotype network for E in Prevalence, molecular characterisation and phylogenetic analyses of hydatid cysts and cysticercus tenuicollis isolates and first report of E. canadensis (G6/G7) in wild boars in Bingol province, Türkiye

Fig. 3. Haplotype network for E. canadensis (G6/G7) using cox1 gene (616 bp) sequences of different countries. The E. canadensis (G6/G7) isolate obtained in this investigation (Hap_01) and the sequences identified as G7 in the Genbank database were utilized. Circle size relative to haplotype data set frequency. Each hatch mark is representative of one nucleotide change. Haplotypes formed by the isolates obtained in this study are marked with an asterisk.

Fig. 1 in Prevalence, molecular characterisation and phylogenetic analyses of hydatid cysts and cysticercus tenuicollis isolates and first report of E. canadensis (G6/G7) in wild boars in Bingol province, Türkiye

Fig. 1. Hydatid cyst image obtained from the lung (A) and liver (B) and C. tenuicollis (C,D) image obtained from its mesentery of wild boar.

Fig. 2. Haplotype network constructed using cox1 in Prevalence, molecular characterisation and phylogenetic analyses of hydatid cysts and cysticercus tenuicollis isolates and first report of E. canadensis (G6/G7) in wild boars in Bingol province, Türkiye

Fig. 2. Haplotype network constructed using cox1 (744 bp) gene sequences of T. hydatigena. Seven haplotypes formed by the T. hydatigena isolates obtained in this study: (Hap 1-Hap 7). Circle size relative to haplotype data set frequency. Each hatch mark is representative of one nucleotide change. Haplotypes formed by the isolates obtained in this study are marked with an asterisk.