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35 results for “Ornithodoros”
Bloodmeal metabarcoding of the argasid tick (Ornithodoros turicata Dugès) reveals extensive vector-host associations
<p>Molecular methods to understand host feeding patterns of arthropod vectors are critical to assess exposure risk to vector-borne disease and unveil complex ecological interactions. We build on our prior work discovering the utility of PCR-Sanger sequencing bloodmeal analysis that work well for soft ticks (<em>Acari: Argasidae</em>), unlike for hard ticks (<em>Acari: Ixodidae</em>), thanks to their unique physiology that retains prior bloodmeals for years. Here, we apply bloodmeal metabarcoding using amplicon deep sequencing to identify multiple host species in individual <em>Ornithodoros turicata</em> soft ticks collected from two natural areas in Texas, United States. Of 788 collected <em>O. turicata</em>, 394 were evaluated for bloodmeal source via metabarcoding, revealing 27 different vertebrate hosts (17 mammals, 5 birds, 1 reptile, and 4 amphibians) fed upon by 274 soft ticks. Information on multiple hosts was derived from 167 individual <em>O. turicata</em> (61%). Metabarcoding revealed mixed vertebrate bloodmeals in <em>O. turicata</em> while same specimens yielded only one vertebrate species using Sanger sequencing. These data reveal wide host range of <em>O. turicata</em> and demonstrate the value of bloodmeal metabarcoding for understanding the ecology for known and potential tick-borne pathogens circulating among humans, domestic animals and wildlife such as relapsing fever caused by <em>Borrelia turicatae</em>. Our results also document evidence of prior feeding on wild pig from an off-host soft tick for the first time in North America; a critical observation in the context of enzootic transmission of African swine fever virus if it were introduced to the US. This research enhances our understanding of vector-host associations and offers a promising perspective for biodiversity monitoring and disease control strategies.</p>
Figure 4 in Ornithodoros faccinii n. sp. (Acari: Ixodida: Argasidae) parasitizing the frog Thoropa miliaris (Amphibia: Anura: Cycloramphidae) in Brazil
Figure 4 Scanninc electron microscopy of nymphs of Ornithodoros faccinii n. sp. A. Idiosoma, dorsal view. B. Idiosoma, ventral view, showinc the preanal croove reachinc the sides of the body (white arrow). C. Genital primordium (white arrow) on the ventral idiosoma. D. Capitulum. E. Tarsi I and U-shaped capsule (white arrow), partially covered by a V-shaped membrane. Scale bars: A. 500 μm; B. 500 μm; C. 250 μm; D. 100 μm; E. 100 μm.
Figure 1 in Ornithodoros faccinii n. sp. (Acari: Ixodida: Argasidae) parasitizing the frog Thoropa miliaris (Amphibia: Anura: Cycloramphidae) in Brazil
Figure 1 Scanninc electron microscopy of idiosoma and capitulum of larvae of Ornithodoros faccinii n. sp. A. Idiosoma, dorsal view. B. Part of basis capituli and hypostome. C. Idiosoma, ventral view. D. Dorsal plate. E. Detail of ventral idiosoma, showinc the pair of setae VPL (ventral posterolateral) (black arrow). Scale bars: A. 500 μm; B. 50 μm; C. 500 μm; D. 100 μm; E. 250 μm.
Figure 3 in Ornithodoros faccinii n. sp. (Acari: Ixodida: Argasidae) parasitizing the frog Thoropa miliaris (Amphibia: Anura: Cycloramphidae) in Brazil
Figure 3 Scanninc electron microscopy of cnatosoma and tarsus of larvae of Ornithodoros faccinii n. sp. A. Capitulum, ventral view. B. Details of capitulum showinc small spurs at the base of hypostome in the lateral position (black arrow). C. Detail of hypostome, palpi and chelicerae. D. Trochanter of palpi with 11 short spurs in the inner side, some of them are bifid (black arrow). E. Tibiotarsus of palpi. F. Hypostome with dental formula 3/3 in the anterior third, and then 2/2 posteriorly to the base. G. Tarsi I. Scale bars: A. 100 μm; B. 500 μm; C. 25 μm; D. 15 μm; E. 15 μm; F. 10 μm; G. 50 μm.
Figure 2 in Ornithodoros faccinii n. sp. (Acari: Ixodida: Argasidae) parasitizing the frog Thoropa miliaris (Amphibia: Anura: Cycloramphidae) in Brazil
Figure 2 Larvae of Ornithodoros faccinii n. sp. A. Chaetotaxy of dorsal idiosoma: DAL (dorsal anterolateral setae), DC (dorsal central setae), DPL (dorsal posterolateral setae). B. Chaetotaxy of ventral idiosoma: ST (sternal setae), CA (circumanal setae), VPL (ventral posterolateral setae). C. Chaetotaxy of tarsus I, A (anterior), DM (dorsomedian), PC (paracapsular), PM (posteromedian), B (basal), AV (anteroventral), MV (midventral), BV (basiventral), PL (posterolateral). D. Licht microcraph of tarsus I, capsule of Haller's orcan. Scale bars: A and B. 100 μm; C. 50 μm; D. 20 μm.
Figure 5 in Ornithodoros faccinii n. sp. (Acari: Ixodida: Argasidae) parasitizing the frog Thoropa miliaris (Amphibia: Anura: Cycloramphidae) in Brazil
Figure 5 Phylocenetic tree based on the 16S rDNA ticks. The alicnment was produced usinc Clustal X and the tree was inferred by means of the MP method with 500 replicates of random addition taxa. The species Ixodes holocyclus and Ixodes uriae were used as outcroup. The Bayesian support (posterior probability) values are derived from 1,000,000 replicates.
Fig. 5 in Population structure of the soft tick Ornithodoros maritimus and its associated infectious agents within a colony of its seabird host Larus michahellis
Fig. 5. Spatial autocorrelation in the total tick number of counted nests, measured as Moran's I, across three distance classes: a, 1st visit; b, 2nd visit; c, 3rd visit; d, 4th visit; e, 5th visit; f, 6th visit. Circles indicate the autocorrelation coefficients. The same results were obtained with female count numbers.
Fig. 2 in Population structure of the soft tick Ornithodoros maritimus and its associated infectious agents within a colony of its seabird host Larus michahellis
Fig. 2. Histogram presenting the mean number of ticks observed in all nests over time. Bars represent mean standard errors of the total number of ticks.
Fig. 3 in Population structure of the soft tick Ornithodoros maritimus and its associated infectious agents within a colony of its seabird host Larus michahellis
Fig. 3. Boxplot representations of tick numbers in counted and collected nests over time: a, females only; b, males only; c, nymphs. The box shows the median as a line across the middle and the quartiles (25th and 75th percentiles) at either end. Extremities represent the minimal and maximal values and circles represent outliers.
Fig. 1 in Population structure of the soft tick Ornithodoros maritimus and its associated infectious agents within a colony of its seabird host Larus michahellis
Fig. 1. Map showing the position of the 30 tracked nests on Carteau Island, in the Camargue region of France (represented by the red point on the bottom right map). Orange points represent the 15 nests in which ticks were counted and released. The green points are those nests where all ticks were counted and collected. Stars within the points represent the nests in which ticks were used for the screening of infectious agents. Boxes indicate the number of ticks screened and the detected infectious agents: Ana: Anaplasma spp.; Bab: Babesia spp.; Bar: Bartonella spp.; Bor: Borrelia spp.; Cox: Coxiella-like symbiont; Fra: Francisella-like symbiont; Ri: Rickettsia helvetica; Ri-like: Rickettsia-like symbiont. (For interpretation of the references to colour in this figure legend, the reader is referred to the web version of this article.)
Fig. 4 in Population structure of the soft tick Ornithodoros maritimus and its associated infectious agents within a colony of its seabird host Larus michahellis
Fig. 4. Spatial autocorrelation in total tick number estimated by Moran's I (Sokal and Oden, 1978). Data are from the first visit in the colony and include nests of both treatments. Ten distance classes representing 10 m between marked nests have been defined. No index value was significantly different from zero. The same results were obtained using female count data only (results not shown).
Fig. 2. Ornithodoros huajianensis n in Ornithodoros (Ornithodoros) huajianensis sp. nov. (Acari, argasidae), a new tick species from the Mongolian marmot (Marmota bobak sibirica), Gansu province in China
Fig. 2. Ornithodoros huajianensis n. sp. (female, holotype): E) Tarsi I ∼ IV; F) Spiracle plate; G) genital apron.
Fig. 4. Ornithodoros huajianensis n in Ornithodoros (Ornithodoros) huajianensis sp. nov. (Acari, argasidae), a new tick species from the Mongolian marmot (Marmota bobak sibirica), Gansu province in China
Fig. 4. Ornithodoros huajianensis n. sp. (nymph, paratype): A) ventral view, entire; B) Coxa I ∼ IV; C) basis capitulum; D) tarsi II and IV; E) Spiracular plate.
Influence of endosymbionts on the reproductive fitness of the tick Ornithodoros moubata tested through elimination of the microbiota using antibiotic treatments
<p class="MsoNoSpacing">Over the past ten years, many studies demonstrated the crucial role of the tick microbiome in tick biology. The soft tick <em>Ornithodoros moubata</em> is a hematophagous ectoparasite of Suidae particularly known to transmit the African swine fever virus. Its bacterial microbiota is characterized by a high prevalence of <em>Francisella</em>-like and <em>Rickettsia</em> endosymbionts. The present study aims to better understand the potential influence of the microbiota on the reproductive fitness of <em>O. moubata</em>. A total of 132 adult female ticks were treated using gentamycin or rifampicin added to the blood meal. Half of the ticks also received a supplementation with B vitamins to address the nutritional role of endosymbionts. Over two periods of 50 days, several traits related to reproductive fitness were monitored to investigate the importance of <em>Francisella</em> and <em>Rickettsia</em> for those traits. It appeared that most of the considered reproductive parameters were not affected. However, antibiotic treatments induced an increase in the tick survival indicating a potential fitness cost of harboring endosymbionts for ticks during the reproduction period. Similarly, 366 first-stage nymphs of <em>Ornithodoros moubata</em> were exposed to the same treatments for molecular quantification of both endosymbionts. Results from qPCR suggested that treatments produced a bacteriostatic effect on endosymbionts without fully eliminating <em>Francisella</em> or <em>Rickettsia</em>.</p>
Influence of endosymbionts on the reproductive fitness of the tick Ornithodoros moubata tested through elimination of the microbiota using antibiotic treatments
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Bloodmeal metabarcoding of the argasid tick (Ornithodoros turicata Dugès) reveals extensive vector-host associations
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Development of twenty-four microsatellite markers for Afrotropical Ornithodoros ticks
<p><strong>Background: </strong>Soft ticks of the genus <em>Ornithodoros</em> are responsible for the maintenance and transmission of the <em>African swine fever </em>(ASF)<em> virus</em> in the sylvatic and domestic viral cycles in Southern Africa. They are also the main vectors of <em>Borrelia</em> species causing relapsing fevers. Currently, no genetic markers are available for Afrotropical <em>Ornithodoros </em>ticks. As ASF spreads globally, such markers are needed to assess the role of ticks in the emergence of new outbreaks. The aim of this study was to design microsatellite markers that could be used for ticks of the <em>Ornithodoros moubata</em> complex, particularly <em>Ornithodoros phacochoerus</em>, to assess population structure and tick movements in ASF endemic areas.</p> <p><strong>Methods: </strong>One hundred and fifty-one markers were designed using the <em>O. moubata </em>and <em>O. porcinus</em> genomes after elimination of repeated sequences in the genomes. All designed markers were tested on <em>O. phacochoerus </em>and <em>O. porcinus </em>DNA to select the best markers.</p> <p><strong>Results:</strong> Twenty-four microsatellite markers were genotyped on two populations of <em>O. phacochoerus</em> and on few individuals from four other <em>Ornithodoros</em> species. Nineteen markers were selected to be as robust as possible for population genetic studies on <em>O. phacochoerus</em>.</p> <p><strong>Conclusions:</strong> The microsatellite markers developed here represent the first genetic tool to study nidicolous populations of Afrotropical <em>Ornithodoros</em>. This dataset contains the genotyping results obtained for all twenty-four markers tested.</p>
Development of twenty-four microsatellite markers for Afrotropical Ornithodoros ticks
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FIGURES 11–15 in Description of nymphal instars of Ornithodoros mimon Kohls, Clifford & Jones, 1969 (Acari: Argasidae)
FIGURES 11–15. Scanning electron microscopy of Ornithodoros mimon, third nymphal instar (N3): 11. Capitulum, median concavity apex on of hypostome arrowed, integumental ridge-like extension in internal margin of the article I of palpi (arrow); 12. Idiosoma dorsal view, disc arrowed; 13. Idiosoma ventral view, genital primordium arrowed; 14. Spiracular plate, semicircular in shape (arrow); 15. Tarsus I and Haller's organ, aperture of capsule arrowed. Scale bars: 11–150 µm; 12–1000 µm; 13–500 µm; 14–50µm; 15–100µm.
FIGURES 7–10 in Description of nymphal instars of Ornithodoros mimon Kohls, Clifford & Jones, 1969 (Acari: Argasidae)
FIGURES 7–10. Scanning electron microscopy of Ornithodoros mimon, second nymphal instar (N2): 7. Capitulum, apex of hypostome with a median concavity, integumental ridge-like extension in internal margin of the article I of palpi arrowed; 8. Idiosoma dorsal view, disc arrowed; 9. Idiosoma ventral view, genital primordium apparent (arrow); 10. Tarsus I and Haller's organ. Scale bars: 7–150 µm; 8–9, 500 µm; 10–100 µm.
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