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Fig. 3 in Tick abundance and life-stage segregation on the American black bear (Ursus americanus)

Fig. 3. Photograph of a bear with severe sarcoptic mange. Note the high loss of fur and thickened skin on the ears, face, and along the sides of the body and higher amounts of fur remaining along the spine and lower limbs. This pattern of hair loss and thickened crusting skin is typical for bears with moderate to severe cases of sarcoptic mange in Pennsylvania, with mild cases also frequently exhibiting higher hair loss and clinical signs of sarcoptic mange on the face and front regions of the body.

Fig. 2a in Tick abundance and life-stage segregation on the American black bear (Ursus americanus)

Fig. 2a. Diagram of tick abundance on American black bears, based on 17 body regions surveyed on black bears from June 2018–December 2019 in Pennsylvania, USA. Figure colors based on percentage of observed tick presence out of all observations of that body region (table), to represent where ticks were most frequently observed within the body regions surveyed. Darker colors indicate higher percentages of observations when ticks were present and lighter colors indicate lower percentages of observations that had ticks present in that body region. Body location descriptors- A: ear; B: cheek; C: neck; D: upper spine; E: lower spine; F: chest; G: front outer leg; H: front inner leg; I: front axillary region; J: front inner toes; K: stomach; L: hip; M: hind outer leg; N: hind inner leg; O: hind axillary region; P: hind inner toes; Q: muzzle. (For interpretation of the references to color in this figure legend, the reader is referred to the Web version of this article.)

Fig. 1 in Tick abundance and life-stage segregation on the American black bear (Ursus americanus)

Fig. 1. Map of capture locations for bears surveyed for tick burden in Pennsylvania from June 2018–December 2019.

Fig. 2. Macroscopic examination. A in Exo-erythrocytic stages of Haemoproteus sp. in common buzzard (Buteo buteo): A histopathological and molecular study

Fig. 2. Macroscopic examination. A pale enlarged liver (Li); B hyperplastic nodules on the surface of the large spleen (S), inflated kidneys (K), and hypostatic congestion of left lung (Lu).

Fig. 5 in Exo-erythrocytic stages of Haemoproteus sp. in common buzzard (Buteo buteo): A histopathological and molecular study

Fig. 5. Maximum-likelihood tree analysis based on partial cytb gene sequences (433 bp) of Haemoproteus from the studied sequence (linage BUTBUT15) and other sequences obtained from MalAvi database. Numbers on the branches indicate the percent of replicates that reproduced the topology for each clade. The percentages of replicate trees in which the associated taxa clustered together in the bootstrap test (1000 replicates) are shown next to the branches. Black circle indicates sequence obtained from the study.

Fig. 1 in Exo-erythrocytic stages of Haemoproteus sp. in common buzzard (Buteo buteo): A histopathological and molecular study

Fig. 1. Gametocytes of haemosporidians (arrows) from the blood of the common buzzards. A-C mature macrogametocytes of L. buteonis in fusiform host cells; A host cell nucleus is not distorted but displaced laterally; B&C host cell nucleus is lateral and flattened; D young gametocyte of Haemoproteus. Giemsa stained thin blood films. Scale bar = 10 μm.

Fig. 4 in Exo-erythrocytic stages of Haemoproteus sp. in common buzzard (Buteo buteo): A histopathological and molecular study

Fig. 4. Megalomeront of Haemoproteus sp. (linage BUTBUT15) from the kidney of a common buzzard. A&B same megalomeront of different magnifications (arrows). The structure is covered with a semi-thick capsule-like wall and contained highly eosinophilic irregularly-shaped cytomeres which have merozoites. Note that the host cell nucleus is not visible inside or close to megalomeront. Scale bars = 200 μm (A); 80 μm (B).

Fig. 3 in Exo-erythrocytic stages of Haemoproteus sp. in common buzzard (Buteo buteo): A histopathological and molecular study

Fig. 3. Meronts of Haemoproteus sp. (linage BUTBUT15) from the lung of a common buzzard. A-D different shapes of pulmonary meronts (arrows). Each meront is surrounded by a thin wall and contained numerous basophilic round to oval merozoites. Note that the host cell nucleus is not visible in meronts. Scale bar = 40 μm.

Fig. 6 in New data on Thelohanellus nikolskii Achmerov, 1955 (Myxosporea, Myxobolidae) a parasite of the common carp (Cyprinus carpio, L.): The actinospore stage, intrapiscine tissue preference and molecular sequence

Fig. 6. Phylogenetic position of Thelohanellus nikolskii spores from the fins and scales of common carp based on SSU rDNA analysis by the Maximum Likelihood algorithm. Myxobolus cerebralis was used as the outgroup. Bootstrap values are given at the nodes. The scale-bar indicates the number of expected substitutions per site.

Fig. 5 in New data on Thelohanellus nikolskii Achmerov, 1955 (Myxosporea, Myxobolidae) a parasite of the common carp (Cyprinus carpio, L.): The actinospore stage, intrapiscine tissue preference and molecular sequence

Fig. 5. Microphotograph of fresh, unstained actinospore of Aurantiactinomyxon type (AUM5) from Nais sp. Insert – apical view of spore with protruding polar capsules.

Fig. 7 in New data on Thelohanellus nikolskii Achmerov, 1955 (Myxosporea, Myxobolidae) a parasite of the common carp (Cyprinus carpio, L.): The actinospore stage, intrapiscine tissue preference and molecular sequence

Fig. 7. Schematic illustration of T. nikolskii life cycle: Aurantiactinomyxon-type actinospores (A) infect the vertebrate host C. carpio (V) in which they develop myxospores (M) that infect the invertebrate host Nais sp. (I).

Fig. 2. A in New data on Thelohanellus nikolskii Achmerov, 1955 (Myxosporea, Myxobolidae) a parasite of the common carp (Cyprinus carpio, L.): The actinospore stage, intrapiscine tissue preference and molecular sequence

Fig. 2. A: Section of an infected fin, containing T. nikolskii cysts, stained with hematoxilin-eosin. Cartilage of finray (cf) is next to the cyst. Plasmodium (p) is in the achromatic tegument, mature myxospores (s) are in the middle, sporoblasts (sb) are at the edges. Around the plasmodium, there is a thick connective tissue (ct) layer, containing cartilaginous elements (c). Multilayer epithelium (e) is the outer layer. B: T. nikolskii myxospores from the plasmodium.

Fig. 4. A in New data on Thelohanellus nikolskii Achmerov, 1955 (Myxosporea, Myxobolidae) a parasite of the common carp (Cyprinus carpio, L.): The actinospore stage, intrapiscine tissue preference and molecular sequence

Fig. 4. A: Cross section of infected scales, stained with hematoxilin-eosin. The plasmodia (p) are filled with myxospores (s) and are surrounded by cartilaginous tissue (c) of the scales, covered by the epithelium layer (e). B: T. nikolskii myxospores from a plasmodium in the scale.

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Fig. 2 in Lungworms (Metastrongylus spp.) and intestinal parasitic stages of two separated Swiss wild boar populations north and south of the Alps: Similar parasite spectrum with regional idiosyncrasies

Fig. 2. Wild boar lung with massive trauma after bullet penetration and visible bone fractures (A), dense nodule of the lobus caudalis dexter (B), and accumulation of nematodes in a bronchus (C).

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Fig. 3 in Lungworms (Metastrongylus spp.) and intestinal parasitic stages of two separated Swiss wild boar populations north and south of the Alps: Similar parasite spectrum with regional idiosyncrasies

Fig. 3. Caudal ends of the 5 Metastrongylus species identified in this study: M. apri female (A) and male (B), M. asymmetricus female (C) and male (D), M. confusus female (E) and male (F), M. pudendotectus female (G) and male (H), M. salmi female (I) and male (J).

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Fig. 1 in Lungworms (Metastrongylus spp.) and intestinal parasitic stages of two separated Swiss wild boar populations north and south of the Alps: Similar parasite spectrum with regional idiosyncrasies

Fig. 1. Map of Switzerland with sampling areas for the northern (Cantons of Aargau (AG), Schaffhausen (SH), Thurgau (TG) and Zürich (ZH)) and the southern (Canton of Ticino (TI)) wild boar population. N: number of lungs sampled.

Fig. 1 in Genetic characterisation of cercarial stages of Choanocotyle Jue Sue and Platt, 1998 (Digenea: Choanocotylidae) in a native Australian freshwater snail, Isidorella hainesii (Tryon)

Fig. 1. Cercaria of Choanocotyle hobbsii. A. Ventral view of whole mount. Scale bar 100 μm. B. Stylet. Scale bar 10 μm.

Figs 21–24 in Redescription of Omophoita octoguttata (Coleoptera: Chrysomelidae) and its immature stages, with notes on life history

Figs 21–24. Omophoita octoguttata (Fabricius, 1775), pupa, habitus: 21, dorsal; 22, ventral; 23, cocoons made from soil matter with pupa; 24, interior of the cocoon, pupa removed. Scale bar = 1 mm.

Figs 19, 20 in Redescription of Omophoita octoguttata (Coleoptera: Chrysomelidae) and its immature stages, with notes on life history

Figs 19, 20. Omophoita octoguttata (Fabricius, 1775), mature larva: 19, head, frontal view (DOS, dorsoepicranial setae; POS, paraocellar setae; PFS, posterofrontal setae; EFS, externofrontal setae; AFS, anterofrontal setae; EES, externoepicranial setae); 20, lateral habitus. Scale bar = 1 mm.

Figs 16–18 in Redescription of Omophoita octoguttata (Coleoptera: Chrysomelidae) and its immature stages, with notes on life history

Figs 16–18. Omophoita octoguttata (Fabricius, 1775): 16, terrarium used for the rearing; 17, clutch of eggs buried in soil within the terrarium;18, egg. Scale = 1 mm.