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opencc-by-4.0Nov 2015View details →

Fig. 2 in Pseudorhadinorhynchus samegaiensis (Acanthocephala: Echinorhynchida: Illiosentidae) Uses the Amphipod Jesogammarus (Annanogammarus) fluvialis as an Intermediate Host in a Stream of the Lake Biwa Basin, Central Japan

Fig. 2. Developmental stages of Pseudorhadinorhynchus samegaiensis. A, Male acanthella; B, early male cystacanth with part of proboscis and copulatory bursa everted, same individual as "c" in Fig. 1B; C, early female cystacanth; D, fully developed male cystacanth with everted proboscis; E, fully developed female cystacanth with everted proboscis; F, everted proboscis of fully developed female cystacanth (E). Scale bars: A, 300 µm; B–E, 500 µm; F, 200 µm.

Fig. 6 in Pseudoleucochloridium ainohelicis nom. nov. (Trematoda: Panopistidae), a Replacement for Glaphyrostomum soricis Found from Long-Clawed Shrews in Hokkaido, Japan, with New Data on its Intermediate Hosts

Fig. 6. The egg of Pseudoleucochloridium ainohelicis nom. nov. in the gravid adult. The left end is an operculum. An arrow indicates the notch of eggshell. A miracidium is visible inside. Scale bar 10 µm.

Fig. 4 in Pseudoleucochloridium ainohelicis nom. nov. (Trematoda: Panopistidae), a Replacement for Glaphyrostomum soricis Found from Long-Clawed Shrews in Hokkaido, Japan, with New Data on its Intermediate Hosts

Fig. 4. The cercaria and metacercaria of Pseudoleucochloridium ainohelicis nom. nov. from Ainohelix editha. Both of the drawings are in ventral view. A) Cercaria. Scale bar 100 µm; B) Metacercaria. Scale bar 500 µm.

Fig. 1 in Pseudoleucochloridium ainohelicis nom. nov. (Trematoda: Panopistidae), a Replacement for Glaphyrostomum soricis Found from Long-Clawed Shrews in Hokkaido, Japan, with New Data on its Intermediate Hosts

Fig. 1. Frequencies of cox1 haplotypes and their statistical parsimony network in Pseudoleucochloridium ainohelicis nom. nov. All of the twelve isolates were collected in Asahikawa. The size of circles indicates the frequency of the haplotypes. Small circles show hypothetical haplotypes. The shaded circle represents the hypothetical ancestor.

Fig. 5 in Pseudoleucochloridium ainohelicis nom. nov. (Trematoda: Panopistidae), a Replacement for Glaphyrostomum soricis Found from Long-Clawed Shrews in Hokkaido, Japan, with New Data on its Intermediate Hosts

Fig. 5. The adult of Pseudoleucochloridium ainohelicis nom. nov. from Sorex unguiculatus. The drawing is in ventral view. The large suckers, M-shaped configuration of uterus, and terminally-positioned genital pore are characteristic of the genus. Scale bar 500 µm.

opencc-by-4.0Apr 2024View details →

Fig. 2 in A first report of PSeUDOSUCCInea COlUMella (Say, 1817), an alien intermediate host for liver fluke, in Malawi

Fig. 2 Conchological and anatomical comparison of Pseudosuccinea columella (top row) and Radix natalensis (bottom row). a–d P.columella conchology (a, b), shell microsculpture of the black square hatched area (c) and radular teeth (d) e–h R. natalensis conchology (e, f), shell microsculpture of the black square hatched area (g) and radular teeth (h). Although there is minor variation in the shape of the inner cusp of the first lateral teeth, the discriminatory feature is the periostracum's spiral ridges

opencc-by-4.0Apr 2024View details →

Fig. 1 in A first report of PSeUDOSUCCInea COlUMella (Say, 1817), an alien intermediate host for liver fluke, in Malawi

Fig. 1 Sketch maps of the distribution of Pseudosuccinea columella in Mangochi (a), Chikwawa (b) and Nsanje (c) Districts, southern Malawi. Red circles indicate HUGS survey sites where P. columella was found; grey circles are surveyed sites where this snail was not found. The locations are: Mangochi 1 (− 14.31373°, 35.14174°); Chikwawa 1 (− 16.03759°, 34.84091°); Nsanje 4 (− 16.88780°, 35.27475°); Nsanje 5 (− 16.92985°, 35.26552°) with corresponding location photograph. Note that the panorama image of Mangochi 1 clearly shows the stream, flowing left to right, directly connected to Lake Malawi. HUGS, Hybridisation in UroGenital Schistosomiasis (project)

opencc-by-4.0Dec 2014View details →

Fig. 3 in Gastric nematode diversity between estuarine and inland freshwater populations of the American alligator (Alligator mississippiensis, daudin 1802), and the prediction of intermediate hosts

Fig. 3. Prey content species richness accumulation curves based on 1000 randomizations using Estimate 9.1.0. Data obtained from stomach flushing or necropsy of American alligators from (A) coastal or (B) inland habitats between 2008 and 2011. The black broken line (- -) represents the upper 95% confidence level, and the broken dotted broken line (- · -) represents the lower 95% confidence level of the species accumulation curve. The slow approach to the asymptote in coastal habitats suggests prey contents of sampled alligators did not capture all probable prey. The asymptote of inland alligators slowly begins to plateau, which may suggest our sampling efforts were close to capturing most of the probable prey of alligators.

opencc-by-4.0Dec 2014View details →

Fig. 2 in Gastric nematode diversity between estuarine and inland freshwater populations of the American alligator (Alligator mississippiensis, daudin 1802), and the prediction of intermediate hosts

Fig. 2. Nematode species richness accumulation curve (A) and Coleman rarefaction curve (B) based on 1000 randomizations using Estimate 9.1.0. The black broken line (- -) represents the upper 95% confidence level, and the broken dotted broken line (- · -) represents the lower 95% confidence level of the species accumulation curve (A). Upper and lower Coleman standard deviations are represented by solid black lines (B). Data obtained from stomach flushing or necropsy of American alligators from Florida and Georgia between 2008 and 2011. The rapid approach to the asymptote suggests we captured all possible species of alligator nematodes.

opencc-by-4.0Apr 2016View details →

Fig. 2 in First identification of Echinococcus multilocularis in rodent intermediate hosts in Sweden

Fig. 2. Macroscopic photos of rodent livers containing Echinococcus multilocularis metacestode lesions. The ruler in each picture is in millimeters. (A) Liver from Microtus agrestis with one lesion that contained protoscoleces. (B) Liver from Arvicola amphibius with multiple lesions that did not contain protoscoleces. (C) Liver from Arvicola amphibius with multiple lesions that did contain protoscoleces. (D) Liver from Arvicola amphibius. Arrow points to the only lesion examined for protoscoleces, which were absent.

opencc-by-4.0Apr 2016View details →

Fig. 1 in First identification of Echinococcus multilocularis in rodent intermediate hosts in Sweden

Fig. 1. Study areas and positive findings of E. multilocularis in southern Sweden at the beginning of the study, 2013. Boxes show study areas and stars indicate where positive foxes/ fox fecal samples had been found. Circles encompass the study areas where rodents positive for E. multilocularis were captured. The lines are county boundaries. (CRS: WGS 84, QGIS 2.12.3).

opencc-by-4.0Apr 2019View details →

Fig. 1 in Evidence of red panda as an intermediate host of Toxoplasma gondii and Sarcocystis species

Fig. 1. Sarcocysts and Toxoplasma gondii cysts in red panda or mice. A: Tissue cysts, leg muscle, red panda. Two oval cysts (arrow) were observed in the skeletal muscle cell. The walls of the two cysts (arrowhead) were deeply stained by eosin. Red panda, H&E. B: Partial magnification of figure A. a, The wall of the cyst was clearly and deeply stained by eosin. b, The bradyzoites were like cresent or banana, they were arranged in packets (arrowhead). c, Necleus of host cell. C: Tissue cyst (arrow) was cross reacted with T. gondii, the cysts were separated by septa and formed many compartments (arrowhead), leg muscle. T. gondii antibody, red panda, IHC. D: Tissue cysts of T. gondii in brain of mouse (arrows), brain squash, unstained, 75DPI. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)

opencc-by-4.0Feb 2021View details →

Figure 1 in Molecular data on Phyllodistomum macrocotyle (Digenea: Gorgoderidae) from an intermediate host Dreissena polymorpha (Bivalvia: Dreissenidae) in the Northern Dvina River Basin, Northwest Russia

Figure 1. Map of the study area: A) Geographic position of the research area (red color frame and red color point); B) The Northern Dvina River Basin (red color flags indicate points where zebra mussels infected with Phyllodistomum macrocotyle were found); C) Habitat of zebra mussel, the Yuras River; D) Trematode sporocysts located within the gills of Dreissena polymorpha.

opencc-by-4.0Feb 2021View details →

Figure 2 in Molecular data on Phyllodistomum macrocotyle (Digenea: Gorgoderidae) from an intermediate host Dreissena polymorpha (Bivalvia: Dreissenidae) in the Northern Dvina River Basin, Northwest Russia

Figure 2. Maximum likelihood phylogeny of Phyllodistomum macrocotyle based on the nuclear dataset (28S rDNA gene fragment). Numbers near nodes are bootstrap support (BS) values of IQ-TREE. Scale bar indicates the branch lengths. The red color indicates our sequence from Northwest Russia.

Fig. 2 in Sensitive, quantitative detection of Besnoitia darlingi and related parasites in intermediate hosts and to assess felids as definitive hosts for known and as-yet undescribed related parasite species

Fig. 2. Coccidia-specific PCR to confirm the presence of DNA of various parasite species used to test the analytic specificity of the BdanjoRT1 real-time PCR. (1) Besnoitia darlingi, (2) B. neotomofelis, (3) B. oryctofelisi, (4) B. besnoiti (Evora isolate), (5) B. bennetti (Texas), (6) B. tarandi (Bt-CA-Quebec1), (7) Toxoplasma gondii, (8) Hammondia hammondi, (9) Neospora caninum, (10) H. heydorni, (11) Cystoisospora felis, (12) C. rivolta, (13) C. burrowsi, (14) C. canis, (15) Sarcocystis cruzi and (16) Crytosporidium parvum. Presence of (17) Giardia duodenalis and (18) Tritrichomonas foetus DNA was shown by amplification using species or genus-specific primers, respectively. C, negative control; M, marker.

Fig. 3 in Sensitive, quantitative detection of Besnoitia darlingi and related parasites in intermediate hosts and to assess felids as definitive hosts for known and as-yet undescribed related parasite species

Fig. 3. Analytic sensitivity (A) and standard curve (B) obtained for the threshold cycle (Cq) values obtained in the BdanjoRT1 real-time PCR using varying amounts of genomic Besnoitia darlingi DNA (approximately equivalent to the DNA content of 10.000 [blue], 1000 [green], 100 [red], 10 [brown] and 1 [black] B. darlingi tachyzoites) diluted in 100 ng/μl mouse DNA. Cq values used for regression are displayed as circles. Results on samples resembling DNA of 0.1 tachyzoite were not included in regression, since only two of four samples had reacted with a Cq value of 37.8 or 38.3 (displayed grey in A and as crosses in B). (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 Sensitive, quantitative detection of Besnoitia darlingi and related parasites in intermediate hosts and to assess felids as definitive hosts for known and as-yet undescribed related parasite species

Fig. 1. Location of the primers and the probe of the Besnoitia darlingi/B.neotomofelis /B. oryctofelisi-specific real-time PCR assay BdanjoRT1 within the ITS-1 region of the rRNA gene. The sequences of the ITS-1 region of B. akodoni (AY545987, bold), B. jellisoni (AF076860, bold), B. neotomofelis (HQ909085, bold), B. darlingi (AF489696, bold) and B. oryctofelisi (AY182000, bold), were aligned relative to sequences of other Besnoitia spp. including B. besnoiti from Portugal, Spain and Germany, B. bennetti reported from the USA and Belgium, B. tarandi from Canada and Finland and those of Neospora caninum, Hammondia heydorni, Toxoplasma gondii and H. hammondi by using Clustal V (DNAStar, Madisin, Wisconsin, USA). Deletions and substitutions in the sequences relative to and within the clade of B. acodoni, B. jellisoni, B. neotomofelis, B. darlingi and B. oryctofelisi are indicated by black background. Sequences of the primer BdanjoRev and the Probe Bb11-12 are displayed in their complementary form. The probe Bb11-12 was established for a real-time PCR to detect B. besnoiti, but it is universal and can be used for the detection of all Besnoitia spp. mentioned here.

Fig. 7 in The morphological and molecular identification of the tapeworm, Taenia lynciscapreoli, in intermediate and definitive hosts in Poland

Fig. 7. Large rostellar hooks: A - larvae T. lynciscapreoli from roe deer; B – larvae T. hydatigena from wild boar, C - larvae T. hydatigena from moose.

Fig. 6 in The morphological and molecular identification of the tapeworm, Taenia lynciscapreoli, in intermediate and definitive hosts in Poland

Fig. 6. Phylogenetic tree of Taenia lynciscapreoli haplotypes, constructed by Bayesian inference (BI) analysis using MrBayes version 3.2. The HKY + G + I model was chosen as the best-fitting nucleotide substitution model using JModelTest version 2.1.10 software (Guindon and Gascuel, 2003; Darriba et al., 2012). Sequences of Echinococcus granulosus sensu stricto GenBank accession number AB688619 and Echinococcus multilocularis GenBank accession number AB461413 were used as the outgroup. Analysis was run for 1,000,000 generations, with 250,000 generations discarded as 'burn-in'. Nodal support is indicated as Bayesian posterior probabilities. Sequences generated in this study are shown in bold. The scale bars are proportional to the number of substitutions per site.

Fig. 5 in The morphological and molecular identification of the tapeworm, Taenia lynciscapreoli, in intermediate and definitive hosts in Poland

Fig. 5. Four crowns of T. lynciscapreoli, A – C larvae, D – adult; A – AM1 (32 hooks), B – APS3 (38 hooks), C – APS2 (34 hooks), D – R17 (36 hooks).