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59 results for “Babesia”
Fig. 2 in Molecular characterization of Babesia peircei and Babesia ugwidiensis provides insight into the evolution and host specificity of avian piroplasmids
Fig. 2. Maximum likelihood phylogenetic tree of the ITS-1 (445 bp) and ITS-2 regions sequences (290 bp) of select avian-infecting Babesia lineages. Sequences identified in this study are emphasized in red, and those of other avian-infecting lineages are shown in blue. For each sequence, the following information is provided: morphospecies (individual identification or Genbank code) host species. Branch lengths are drawn proportionally to evolutionary distance (scale bar shown corresponds to both trees). (For interpretation of the references to colour in this figure legend, the reader is referred to the web version of this article.)
Fig. 3 in Molecular characterization of Babesia peircei and Babesia ugwidiensis provides insight into the evolution and host specificity of avian piroplasmids
Fig. 3. Distribution of the phylogenetic groups of avian piroplasmids (based on the 18S rRNA gene) in relation to the phylogeny of avian orders (based on multiple nuclear genes). Avian orders investigated in this study are shown in red, and other avian orders known to host piroplasmids are shown in blue. Avian phylogeny was adapted from Yuri et al. (2013). (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 Molecular characterization of Babesia peircei and Babesia ugwidiensis provides insight into the evolution and host specificity of avian piroplasmids
Fig. 1. Maximum likelihood phylogenetic tree of the 18S rRNA gene sequences (1450 bp) of the studied Babesia lineages. Sequences obtained in this study are emphasized in red, and those of other avian-infecting lineages are shown in blue. For each sequence, the following information is provided: morphospecies (individual identification or GenBank code) host species. For avian-infecting lineages, the host order is indicated with colored circles (see legend). Branch lengths are drawn proportionally to evolutionary distance. (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 Prevalence and co-infection with tick-borne Anaplasma phagocytophilum and Babesia spp. in red deer (Cervus elaphus) and roe deer (Capreolus capreolus) in Southern Norway
Fig. 1. Phylogenetic tree of Babesia isolates and samples of this study (●), based on fragments of 18S rRNA, generated using the Maximum-Likelihood clustering method in MEGA 6 software (1000 replicates; bootstrap values indicated at the nodes). Abbreviations: AU - Austria, BE - Belgium, CA - Canada, DE - Germany, FR - France, HU - Hungary, IT - Italy, JP - Japan, LT - Lithuania, NO - Norway, PL - Poland, RU - Russia, SK - Slovakia, SP - Spain, TU - Turkey, US - United States.
Fig. 1 in Prevalence and distribution of Babesia and Theileria species in roe deer from Spain
Fig. 1. Map of Spain (modified from Morrondo et al., 2017) showing the four ecological areas. Dots represent the presence of Babesia spp. and/or Theileria spp. in each region.
Fig. 2 in Description of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) from southern Florida, USA
Fig. 2. Genetic relationships of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) compared with other Babesia spp. based on near full length 18S rRNA gene sequences. The text in bold blue in the figure represents specimens analyzed in this study. Sequences in light blue are species that have been primarily associated with felid hosts. Green lineages are predominately associated with canid hosts but have been reported in felids. Several sequences derived from domestic cats (i.e., MW578972, PP151898, and PP151899) and wild felids (i.e., HQ187782 and HQ187782) were not included in the analysis because the sequences were short.
Fig. 1 in Description of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) from southern Florida, USA
Fig. 1. Photomicrographs of Babesia coryicola sp. nov., type-material in blood smears from FP222 Florida puma (Puma concolor coryi) (A–C) showing ring and amoeboid trophozoites and FP93 (D) showing a compact ring form.
Fig. 4 in Description of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) from southern Florida, USA
Fig. 4. Genetic relationships of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) compared with other Babesia spp. based on partial cytb gene sequences. The text in bold in the figure represents specimens analyzed in this study.
Fig. 2. A in Prevalence and geographic distribution of Babesia conradae and detection of Babesia vogeli in free-ranging California coyotes (Canis latrans)
Fig. 2. A) PCR positivity (indicated by color) of coyotes (Canis latrans) carcasses recovered (▴) in each county between 2015 and 2019. B) Map of southern California including Los Angeles, Orange, Ventura, San Bernardino, Riverside, and San Diego counties showing B. conradae PCR positivity (indicated by color) in each city where coyote carcasses were recovered. The number of coyotes sampled at each location is indicated by the size of the circle.
Fig. 3 in Prevalence and geographic distribution of Babesia conradae and detection of Babesia vogeli in free-ranging California coyotes (Canis latrans)
Fig. 3. Maximum likelihood phylogenetic tree of Babesia positive coyotes (Canis latrans) collected in California from 2015 to 2019 with 7 different published reference sequences from other Babesia species for comparison. Scale bar represents percent of genetic variation along tree branches. Labels include coyote ID and location found. Alphanumeric values in parenthesis denote published GenBank sequence. Clades in <60% of bootstraps are collapsed.
Fig. 1 in Prevalence and geographic distribution of Babesia conradae and detection of Babesia vogeli in free-ranging California coyotes (Canis latrans)
Fig. 1. Base pair differences in a 70 base pair region of the 18S gene from Babesia conradae DNA sequences isolated from California coyotes (Canis latrans) splenic samples collected between 2015 and 2019 compared to published sequence available in GenBank.
Fig. 2 in First detection and molecular identification of Babesia gibsoni and Hepatozoon canis in an Asiatic wild dog (Cuon alpinus) from Thailand
Fig. 2. Neighbor-joining (NJ) tree of the Hepatozoon partial 18S ribosomal RNA (18S rRNA) gene sequence. Hepatozoon canis (MK144332) was amplified from an Asiatic wild dog in Thailand and analyzed for comparison with other Hepatozoon spp. from the GenBank database. The numbers on branches indicate percent bootstrap support based on 1000 bootstrap replications and only bootstrap values ≥ 50% are shown.
Fig. 1 in First detection and molecular identification of Babesia gibsoni and Hepatozoon canis in an Asiatic wild dog (Cuon alpinus) from Thailand
Fig. 1. Neighbor-joining (NJ) tree of the Babesia partial 18S ribosomal RNA (18S rRNA) gene sequence. Babesia gibsoni (MK144331) was amplified from an Asiatic wild dog in Thailand and analyzed for comparison with other Babesia spp. from the GenBank database. The numbers on branches indicate percent bootstrap support based on 1000 bootstrap replications and only bootstrap values ≥ 50% are shown.
Fig. 6 in Description of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) from southern Florida, USA
Fig. 6. Genetic relationships of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) compared with other Babesia spp. based on partial COX3 gene sequences. The text in bold in the figure represents specimens analyzed in this study.
Fig. 5 in Description of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) from southern Florida, USA
Fig. 5. Genetic relationships of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) compared with other Babesia spp. based on partial COI gene sequences. The text in bold in the figure represents specimens analyzed in this study.
Fig. 3 in Description of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) from southern Florida, USA
Fig. 3. Genetic relationships of Babesia coryicola sp. nov. from Florida pumas (Puma concolor coryi) compared with other Babesia spp. based on partial β-tubulin gene sequences. The text in bold in the figure represents specimens analyzed in this study.
Ecological interactions driving population dynamics of two tick-borne pathogens, Borrelia burgdorferi and Babesia microti
<p><em>Borrelia</em> <em>burgdorferi</em> (<em>Bb</em>) and <em>Babesia</em> <em>microti</em> (<em>Bm</em>) are vector-borne zoonotic pathogens commonly found co-circulating in <em>Ixodes</em> <em>scapularis</em> and <em>Peromyscus</em> <em>leucopus</em> populations. The restricted distribution and lower prevalence of <em>Bm</em> has been historically attributed to lower host-to-tick transmission efficiency and limited host ranges. We hypothesized that prevalence patterns are driven by coinfection dynamics and vertical transmission. We use a multi-year, multiple-location, longitudinal dataset with mathematical modelling to elucidate coinfection dynamics between <em>Bb</em> and <em>Bm</em> in natural populations of <em>P. leucopus</em>, the most competent reservoir host for both pathogens in the eastern USA. Our analysis indicates that, in the absence of vertical transmission, <em>Bb</em> is viable at lower tick numbers than <em>Bm</em>. However, with vertical transmission, Bm is viable at lower tick numbers than <em>Bb</em>. Vertical transmission has a particularly strong effect on <em>Bm</em> prevalence early in the active season while coinfection has an increasing role during the nymphal peak. Our analyses indicate that coinfection processes, such as facilitation of <em>Bm</em> infection by <em>Bb</em>, have relatively little influence on the persistence of either parasite. We suggest future work examines the sensitivity of <em>Bm</em> vertical transmission and other key processes to local environmental conditions to inform surveillance and control of tick-borne pathogens.</p>
Ecological interactions driving population dynamics of two tick-borne pathogens, Borrelia burgdorferi and Babesia microti
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List of tabanid species collected by Lucas et al. (2020) analysed for Babesia spp.
<p>*The list of tabanids was reviewed and corrected in relation to that used by Rodrigues et al. (2022) in the study "Molecular detection of <em>Anaplasma marginale</em> Theiler (Rickettsiales: Anaplasmataceae) in horseflies (Diptera: Tabanidae) in Uruguay" <a href="https://doi.org/10.1038%2Fs41598-022-27067-0" target="_blank" rel="noopener noreferrer">10.1038/s41598-022-27067-0</a></p>
List of tabanid species collected by Lucas et al. (2020) analysed for Babesia spp.
<p>*The list of tabanids was reviewed and corrected in relation to that used by Rodrigues et al. (2022) in the study "Molecular detection of <em>Anaplasma marginale</em> Theiler (Rickettsiales: Anaplasmataceae) in horseflies (Diptera: Tabanidae) in Uruguay" <a href="https://doi.org/10.1038%2Fs41598-022-27067-0" target="_blank" rel="noopener noreferrer">10.1038/s41598-022-27067-0</a></p>
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