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Fig. 2. A in Review of tapeworms of rodents in the Republic of Buryatia, with emphasis on anoplocephalid cestodes

Fig. 2. A neighbour-joining reconstruction of partial cytochrome oxidase I (mtDNA) sequences of Paranoplocephala spp., Andrya rhopalocephala and Neandrya cuniculi from lagomorphs were used as an outgroup. The labels show the GenBank number for each sequence. Values at nodes show the percentage from 10000 bootstrap replicates.

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Fig. 1 in Review of tapeworms of rodents in the Republic of Buryatia, with emphasis on anoplocephalid cestodes

Fig. 1. Study sites in Buryatia. 1-6, Kamensk, Pasolskaya, Ganzurinov, Nizhnaya Ivolga, Verhnaya Berezovka, Utochkina Pad; 7, Maloje Kolesova; 8-10, Barguzin River, Shapen'kovo, Nesteriha; 11-13, Muhorshibir, Sharaldai, Zabaikalsk; 14, Tseremushki.

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Fig. 2 in Tapeworms detected in wolf populations in Central Italy (Umbria and Marche regions): A long-term study

Fig. 2. Neighbor-Joining phylogenetic tree of the sequenced Taenia species and E. granulosus s.s. G3. Maximum Composite Likelihood method, 1000 bootstraps (MEGA11 Software).

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Fig. 1 in Tapeworms detected in wolf populations in Central Italy (Umbria and Marche regions): A long-term study

Fig. 1. Details of sampling and results: number of wolves by region (A); number of positive wolves (B); percentages of positive and negative samples (C); geolocation of parasites (D).

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Figure 2 in Infection caused by the tapeworm Ligula intestinalis (Cestoda, Diphyllobothriidae) in the invasive cyprinid Rutilus rutilus (L., 1758), in three man-made lakes in Algeria

Figure 2. – Spatial and temporal variations of parasitic indices of Ligula intestinalis in Rutilus rutilus in Ghrib, Sekkak and Guenitra dams. P%: Prevalence; A: Parasitic abundance; I: Mean intensity of infection.

opencc-by-4.0Aug 2019View details →

Fig. 2 in Broad tapeworms (Diphyllobothriidae), parasites of wildlife and humans: Recent progress and future challenges

Fig. 2. Microphotographs of permanent slides of diphyllobothriid tapeworms. A – Dibothriocephalus alasensis from Canis familiaris, Hooper Bay, Alaska, March 18, 1958; fixed after relaxation by R. Rausch (MSBP 17029). B – Dibothriocephalus latus from Homo sapiens, Chile, 19 November 2012; contracted clinical sample fixed with 'cold' fixative by T. Weitzel. C – Dibothriocephalus dalliae from C. familiaris, Alaska, 5 November 1970; fixed after relaxation by R. Rausch (MSBP 26232). D – Diphyllobothrium lanceolatum from Erignathus barbatus, Greenland, 7 October 1987; collected by P. Baagoe (SNM). E – Dibothriocephalus cf. nihonkaiensis from Homo sapiens, Newtok, Alaska, 26 March 1967; fixed after relaxation by R. Rausch (MSBP 26244). F – Diphyllobothrium stemmacephalum from Lagenorhynchus acutus, Wellfleet Bay, Cape Cod, Massachusetts, 1998; collected by J.N. Caira. G – Diphyllobothrium mobile from Ommatophoca rossii, Antarctica, 11 August 1901, Deutsche Südpolar- Expedition; collected by E. Dagobert von Drygalski (ZNB 5188). H – Dibothriocephalus ursi from Ursus arctos middendorfi, Karluk Lake, Kodiak Island, 9 October 1952; fixed after relaxation by R. Rausch; paratype (MSBP 3269). I – Schistocephalus sp. from C. familiaris, Newtok, Alaska, 4 April 1958; fixed after relaxation by R. Rausch (MSBP 17939). Acronyms of museum collections: MSBP – Museum of Southwestern Biology, Division of Parasitology, University of New Mexico, Albuquerque, New Mexico, U.S.A.; SNM – Swedish Museum of Natural History, Stockholm, Sweden; ZNB – Zoologische Museum Berlin, Berlin, Germany.

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).

Fig. 4 in The morphological and molecular identification of the tapeworm, Taenia lynciscapreoli, in intermediate and definitive hosts in Poland

Fig. 4. The crown of T. lynciscapreoli; examples of empty spaces, from where hooks have been lost are indicated (arrows).

Fig. 3. A in The morphological and molecular identification of the tapeworm, Taenia lynciscapreoli, in intermediate and definitive hosts in Poland

Fig. 3. A – lung of roe deer with cyst of tapeworm T. lynciscapreoli; B – Cysticercoid of T. lynciscapreoli.

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Fig. 1 in Caryophyllidean tapeworms (Cestoda), Nearctic parasites of fish in Mexico, including description of a new species of Isoglaridacris and the first report of Khawia japonensis, an invasive parasite of common carp (Cyprinus carpio)

Fig. 1. Archigetes sp. 1 from Notropis caliensis, Michoac´an (CNHE 6800) (A, C, F); Archigetes (?) sp. 2 from Notropis nazas, Durango (CNHE 6797) (B, E); Archigetes sp. 3 from Chirostoma sp., Michoac´an (CNHE 6801) (D). A, B – total view, dorsally; C, E – anterior part with scolex; note different position of anterior-most testes and vitelline follicles between C and E; D – total view, ventrally; F – ovarian and uterine region, dorsally. Abbreviations: cs – cirrus-sac; eb – excretory bladder; eg – eggs; esv – external seminal vesicle; lo – loculi; ov – ovary; sr – seminal receptacle; te – testes; vf – vitelline follicles.

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Fig. 3 in Caryophyllidean tapeworms (Cestoda), Nearctic parasites of fish in Mexico, including description of a new species of Isoglaridacris and the first report of Khawia japonensis, an invasive parasite of common carp (Cyprinus carpio)

Fig. 3. Khawia japonensis (Yamaguti, 1934) from Cyprinus carpio, Durango (CNHE 6516). A – total view, ventrally (median preovarian vitelline follicles omitted except for anterior-most follicles); B – anterior end; C – posterior end, ventrally. Abbreviations: cgp – common genital pore; cs – cirrus-sac; Mg – Mehlis' gland; ov – ovary; povf – postovarian vitelline follicles; sd – sperm duct (vas deferens); sr – seminal receptacle; te – testes; ug – uterine glands; ut – uterus; va – vagina; vf – vitelline follicles.

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Fig. 2 in Caryophyllidean tapeworms (Cestoda), Nearctic parasites of fish in Mexico, including description of a new species of Isoglaridacris and the first report of Khawia japonensis, an invasive parasite of common carp (Cyprinus carpio)

Fig. 2. Isoglaridacris brevicollis sp. n. from Catostomus nebuliferus, Durango (CNHE 6802; IPCAS C-885; 2x CNHE 6761) (A–D), Catostomus bernardini, Sonora (CNHE 6796) (E), and Moxostoma astrinum, Jalisco (CNHE 6799) (F); Pseudoglaridacris confusa (Hunter, 1929) from Ictiobus meridionalis, Oaxaca (CNHE 6798) (G). A – total view, ventrally; B – anterior end; C – posterior end, ventrally; D – slightly contracted scolex; E – cirrus-sac with external seminal vesicle, ventrally; F – ovary with overlapping posterior wings, dorsally (uterine loops are omitted at level of ovarian isthmus and more posteriorly); G – total view, dorsally. Abbreviations: cgp – common genital pore; cs – cirrus-sac; eb – excretory bladder; esv – external seminal vesicle; lo – loculi; ov – ovary; povf – postovarian vitelline follicles; sd – sperm duct (vas deferens); te – testes; ut – uterus; va – vagina; vd – vitelline duct; vf – vitelline follicles.

Fig. 11 in Discovering high species diversity of Ophiotaenia tapeworms (Cestoda: Proteocephalidae) of watersnakes (Colubridae) in North America

Fig. 11. Maximum likelihood phylograms of cox1 data (Alignment 4; 549 nt) for selected members of the Proteocephalidae. Bootstrap support from maximum likelihood (ML) and Bayesian inference (BI) nodal support are indicated as ML/BI; values <0.90 (BI) and <70 (ML) are not shown. The scale bar indicates the expected number of substitutions per site. The newly generated sequences are highlighted in bold. Abbreviations of the U.S. states where the samples were collected: AR – Arkansas; MS – Mississippi; OK – Oklahoma. Abbreviations of biogeographical regions: NEA – Nearctic; NEO – Neotropical.

Fig. 9 in Discovering high species diversity of Ophiotaenia tapeworms (Cestoda: Proteocephalidae) of watersnakes (Colubridae) in North America

Fig. 9. Maximum likelihood phylogram based on 28S rDNA data for selected members of the Proteocephalidae. Bootstrap support from maximum likelihood (ML) and Bayesian inference (BI) nodal support are indicated as ML/BI; values <0.90 (BI) and <70 (ML) are not shown. The scale bar indicates the expected number of substitutions per site. The newly generated sequences are highlighted in bold. The hosts are indicated by silhouettes. The sequence of O. europaea obtained from a fish intermediate host is indicated by an asterisk. Abbreviations of the U.S. states where the samples were collected: AR – Arkansas; MS – Mississippi; OK – Oklahoma. Abbreviations of biogeographical regions: NEA – Nearctic; NEO – Neotropical; PAL – Palaearctic.

Fig. 8. Ophiotaenia tkachi n in Discovering high species diversity of Ophiotaenia tapeworms (Cestoda: Proteocephalidae) of watersnakes (Colubridae) in North America

Fig. 8. Ophiotaenia tkachi n. sp. from Nerodia fasciata confluens, host US 952 (MHNG-PLAT-0130134) (A, B, E, F) and N. erythrogaster, host US 1118 (G, H), and O. perspicua La Rue (1911) (C, D) from Nerodia rhombifer rhombifer (US 951), all samples from Oklahoma, USA. A, B – cross sections at the testicular and ovarian level, respectively; C, D – eggs; E–H – unripe eggs (without fully formed oncospheres), drawn in distilled water.

Fig. 10 in Discovering high species diversity of Ophiotaenia tapeworms (Cestoda: Proteocephalidae) of watersnakes (Colubridae) in North America

Fig. 10. Maximum likelihood phylograms of cox1 data (Alignment 3; 1608 nt) for selected members of the Proteocephalidae. Bootstrap support from maximum likelihood (ML) and Bayesian inference (BI) nodal support are indicated as ML/BI; values <0.90 (BI) and <70 (ML) are not shown. The scale bar indicates the expected number of substitutions per site. The newly generated sequences are highlighted in bold. Abbreviations of the U.S. states where the samples were collected: AR – Arkansas; MS – Mississippi; OK – Oklahoma. Abbreviations of biogeographical regions: NEA – Nearctic; NEO – Neotropical.

Fig. 7. Ophiotaenia tkachi n in Discovering high species diversity of Ophiotaenia tapeworms (Cestoda: Proteocephalidae) of watersnakes (Colubridae) in North America

Fig. 7. Ophiotaenia tkachi n. sp. from Nerodia fasciata confluens, host USA 21, Louisiana, USA, holotype (MHNG-PLAT-0063340). A, B – pregravid proglottids, ventral view; C, D – vaginal canal of unusual structure, ventral view (C) and en face view (D).

Fig. 5. Ophiotaenia laruei n in Discovering high species diversity of Ophiotaenia tapeworms (Cestoda: Proteocephalidae) of watersnakes (Colubridae) in North America

Fig. 5. Ophiotaenia laruei n. sp. (A, B) from Nerodia rhombifer rhombifer, Illinois, USA (USNM 1696448) and Ophiotaenia sp. (C) from Thamnophis sirtalis, Michigan, USA (USNM 1351911). A – mature proglottid of holotype, dorsal view; B, C – terminal genitalia, dorsal view.