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Fig. 6 in Morphological and molecular phylogenetic characterization of Sarcocystis kani sp. nov. and other novel, closely related Sarcocystis spp. infecting small mammals and colubrid snakes in Asia

Fig. 6. Mapping of (A) potential heme ligand binding sites and (B) amino acid variability among different lineages of tissue cyst-forming coccidia in the barcode area of the mitochondrial COX1 protein. A) Map of putative heme ligand binding sites (arrowheads) in a protein sequence alignment of selected taxa used in the phylogenetic tree of cox1. Identical/conservative aa positions are highlighted by light background, variable positions and gaps are shown against black background. Helix 1 (H1) is shown partial, starting at position 14 of the global barcode alignment (Pentinsaari et al., 2016); aa sequences of helices 2 (H2) and 6 (H6) are shown in full length, while putative heme binding sites of loop 3–4 (L3-4) were in its anterior part only. Domain boundaries and putative ligand binding sites were derived from COX1 of template organisms Saccharomyces cerevisiae and Bos taurus by sequence alignment against Toxoplasma gondii applying three-dimensional homology modelling of protein structure. The complete alignment of the six helices of the barcode area is shown in Supplementary Fig. S2. Note that aa numbering of the barcode area of the Apicomplexan sequence is different to the global alignment, because the former showed one additional aa and domain boundaries were slightly altered. The nucleotide sequence KC209732 of S. tenella (GenBank) is also registered in the barcode reference database BOLD (accession number JRPAA5858-15; http://boldsystems.org); the aa barcode position 14 (Glycine) shown here corresponds to position 16 of the aa translation of GenBank record KC209732. B) 'Heat map' of aa changes (darker shades of green = more changes, number of changes indicated) in the barcode area among chemically/structurally different aa groups in different lineages of tissue cyst-forming coccidia relative to the COX1 protein sequence of T. gondii. Because helix 1 was truncated, records of aa changes in this area are incomplete.

Fig. 3 in Molecular phylogenetics and systematics of two enteric helminth parasites (Baylisascaris laevis and Diandrya vancouverensis) in the Vancouver Island marmot (Marmota vancouverensis)

Fig. 3. Bayesian consensus phylogram based on Baylisascaris and outgroup alignments of concatenated nuclear sequences (28S, ITS, and ard1) from GenBank and this study (B. laevis). Branch labels represent Bayesian posterior probabilities. Branch lengths are scaled to expected number of substitutions per site. Abbreviations refer to sampling sites (AK = Alaska, ID = Idaho, CT = Connecticut; IL = Illinois; CA = California; WV = West Virginia; ALB = Alberta). See also Table 1.

Fig. 2 in Molecular phylogenetics and systematics of two enteric helminth parasites (Baylisascaris laevis and Diandrya vancouverensis) in the Vancouver Island marmot (Marmota vancouverensis)

Fig. 2. Bayesian consensus phylogram based on Baylisascaris and outgroup alignments of concatenated mitochondrial sequences (12S, cox1, and cox2) from GenBank and this study (B. laevis). Branch labels represent Bayesian posterior probabilities. Branch lengths are scaled to expected number of substitutions per site. Abbreviations refer to sampling sites (AK = Alaska, ID = Idaho, CT = Connecticut; IL = Illinois; CA = California; WV = West Virginia; ALB = Alberta). See also Table 1.

Fig. 1 in Molecular phylogenetics and systematics of two enteric helminth parasites (Baylisascaris laevis and Diandrya vancouverensis) in the Vancouver Island marmot (Marmota vancouverensis)

Fig. 1. Known geographic distributions of Baylisascaris laevis and Diandrya composita in North America.

Fig. 4 in Molecular phylogenetics and systematics of two enteric helminth parasites (Baylisascaris laevis and Diandrya vancouverensis) in the Vancouver Island marmot (Marmota vancouverensis)

Fig. 4. Bayesian consensus phylogram based on Baylisascaris and outgroup alignments of concatenated mitochondrial (12S, cox1, and cox2) and nuclear sequences (28S, ITS, and ard1) from GenBank and this study (B. laevis). Branch labels represent Bayesian posterior probabilities. Branch lengths are scaled to expected number of substitutions per site. Abbreviations refer to sampling sites (AK = Alaska, ID = Idaho, CT = Connecticut; IL = Illinois; CA = California; WV = West Virginia; ALB = Alberta). See also Table 1.

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Fig. 1 in Molecular characterization of Dipetalonema yatesi from the black-faced spider monkey (Ateles chamek) with phylogenetic inference of relationships among Dipetalonema of Neotropical primates

Fig. 1. Macroscopic observation of Dipetalonema yatesi on the capsule of the left kidney (A) and on the parietal peritoneum (B) at the post-mortem examination of a black-faced spider monkey (Ateles chamek).

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Fig. 2 in Molecular characterization of Dipetalonema yatesi from the black-faced spider monkey (Ateles chamek) with phylogenetic inference of relationships among Dipetalonema of Neotropical primates

Fig. 2. Phylogenetic relationships among species of Dipetalonema spp. infecting non-human primates (i.e., Ateles spp., Cebus spp., Lagothrix poeppigii, and Saimiri sciureus) using a concatenated dataset of 1615 base pairs including the 18S of the nuclear ribosomal DNA, 12S of the ribosomal RNA, and cytochrome c oxidase subunit 1 (cox1) of the mitochondrial DNA. The taxa Acanthocheilonema viteae, Litomosoides sigmodontis, and Wuchereria bancrofti were used as outgroups. At each branch, the nodal support is represented by the maximum likelihood percentage above and the Bayesian posterior probability below (the hyphen indicates when support is missing).

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Fig. 3 in Molecular characterization of Dipetalonema yatesi from the black-faced spider monkey (Ateles chamek) with phylogenetic inference of relationships among Dipetalonema of Neotropical primates

Fig. 3. Phylogenetic relationships among species of Dipetalonema using a dataset of 586 base pairs including the partial cytochrome c oxidase subunit 1 (cox1) of the mitochondrial DNA. The black silhouettes of the monkey, tamarin, and camelid indicate the hosts from which the filarioid nematodes were isolated. The taxa Acanthocheilonema viteae, Litomosoides sigmodontis, and Wuchereria bancrofti were used as outgroups. At each branch, the nodal support is represented by the maximum likelihood percentage above and the Bayesian posterior probability below.

Fig. 13 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 13. Morphology of male thoracic sternal plates and associated posterior setae for previously described species of Lemurpediculus, A: Lemurpediculus petterorum Paulian, 1958. B: Lemurpediculus madagascariensis Durden et al. (2018). C: Lemurpediculus claytoni Durden et al., 2017. D: Lemurpediculus verruculosus (Ward, 1951). E: Lemurpediculus robbinsi Durden et al., 2017. Scale bar, 0.1 mm.

Fig. 7 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 7. Lemurpediculus zimmermanni, female, scanning electron micrographs: A, dorsal whole body. B, ventral whole body. Abbreviations: sgp, subgenital plate; sp, spiracle; tc, tibiotarsal claw; tsp, thoracic sternal plate; vs, ventral head spike.

Fig. 5 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 5. Lemurpediculus zimmermanni, stacked photoimages: A, male Holotype, USNMENT00981950, whole body. B, male, Holotype, USNMENT00981950, genitalia. C, female Allotype, USNMENT00981951, whole body.

Fig. 6. Lemurpediculus zimmermanni, A in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 6. Lemurpediculus zimmermanni, A: Ventral head of male Holotype, B: Thoracic sternal plate of Holotype male, C: Genitalia of male Holotype, D: Subgenital plate of female allotype. Abbreviations: ae, anterior endomere; aen, aedeagal endomere; ba, basal apodeme; p, paramere; pe, posterior endomere; ps, pseudopenis.

Fig. 8 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 8. Lemurpediculus gerpi, stacked photoimages: A, male Holotype, USNMENT00981952, whole body. B, male, Holotype, USNMENT00981952, genitalia.

Fig. 10 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 10. Lemurpediculus tsinamanpesotsae, stacked photoimages: A, male Holotype, USNMENT00981954, whole body. B, male, Holotype, USNMENT00981954, genitalia. C, female Allotype, USNMENT00981955, whole body.

Fig. 14 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 14. Morphology of female subgenital plates and associated setae for previously described species of Lemurpediculus, A: Lemurpediculus claytoni Durden et al., 2017. B: Lemurpediculus robbinsi Durden et al., 2017. C: Lemurpediculus verruculosus (Ward, 1951). D: Lemurpediculus petterorum Paulian, 1958. E: Lemurpediculus madagascariensis Durden et al. (2018).

Fig. 2 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 2. Maximum likelihood phylogenetic trees based on A) elongation factor 1α (EF1α), B) cytochrome C oxidase subunit I (COI) and C) internal transcribed spacer 1 (ITS1) sequences. Values next to the branches indicate ultrafast bootstrap support. Tree scale is in substitutions/site. Substitution models were TNe + G4 for EF1α, TPM2+F + I + G4 for COI, and F81 + F + I for ITS1. Abbreviations: F., Fahrenholzia; H., Haematopinus; L., Lemurpediculus.

Fig. 3 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 3. Maximum likelihood phylogenetic tree based on concatenated cytochrome C oxidase subunit I (COI), elongation factor 1α (EF1α) and internal transcribed spacer 1 (ITS1) sequences. Substitution models were TPM2u + F + I + G4 for COI, TIM2e for EF1α and F81 + F + I for ITS1. Values next to the branches indicate ultrafast bootstrap support. Tree scale is in substitutions/site. Abbreviations: L., Lemurpediculus.

Fig. 4 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 4. Lemurpediculus zimmermanni, male, scanning electron micrographs: A, dorsal whole body. B, ventral whole body. Abbreviations sgp, subgenital plate; sp, spiracle; tc, tibiotarsal claw; tsp, thoracic sternal plate; vs, ventral head spike.

Fig. 1 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 1. Sampling sites where cheirogaleids were trapped for collection of lice. Different colours/symbols correspond to the sampled host species/populations, with different shades of blue and green indicating different populations of M. murinus and M. gerpi, respectively. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)

Fig. 12 in Molecular phylogenetics of the sucking louse genus Lemurpediculus (Insecta: Phthiraptera), ectoparasites of lemurs, with descriptions of three new species

Fig. 12. Identifying morphological characters of male genitalia for previously described species of Lemurpediculus, A: Lemurpediculus petterorum Paulian, 1958. B: Lemurpediculus verruculosus (Ward, 1951). C: Lemurpediculus claytoni Durden et al., 2017. D: Lemurpediculus robbinsi Durden et al., 2017. E: Lemurpediculus madagascariensis Durden et al. (2018). Scale bar, 0.1 mm. Abbreviations: as, accessory sclerite; ba, basal apodeme; p, paramere; ndomere; ps, pseudopenis.