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302 results for “cotton”
FIGURE 1 in A review of Gongylonema spp. (Nematoda: Gongylonematidae) in North American rodents with description of a new species from the cotton rat, Sigmodon hispidus (Mammalia: Cricetidae)
FIGURE 1. Drawings of Gongylonema archboldi n. sp. A. Male, anterior end with detail of nerve ring, muscular esophagus and beginning of glandular esophagus and cuticular bosses, internal and surface view. B. Female, anterior end with detail of nerve ring, muscular esophagus and beginning of glandular esophagus and cuticular bosses, internal and surface view in two different figures. C. Male, caudal papillae asymmetrical, pedunculate and variable in number of pre-cloacal and post-cloacal papillae and sessile papillae near tail, ventral view. D. Male, spicules dissimilar and very unequal in length, right spicule boatshaped and left spicule thin, needle-tipped. E. Male, detail of gubernaculum with a cup-shaped base in which the right spicule rests.
FIGURE 2 in A review of Gongylonema spp. (Nematoda: Gongylonematidae) in North American rodents with description of a new species from the cotton rat, Sigmodon hispidus (Mammalia: Cricetidae)
FIGURE 2. Scanning electron micrographs of Gongylonema archboldi n. sp. A. Male, anterior end with prominent cuticular bosses, ventro-lateral view. B. Female, anterior end with more numerous prominent cuticular bosses than the male, ventral view. C. Female, detail of lateral alae, lateral view. D. Female, detail of prominent cuticular bosses.
Subspecies and Distribution. M. c. capensis Schreber, 1776 — S Africa N to Angola, Mozambique, and Zambia. M. c. buechneri Baryshnikov, 2000 — C Asia including Afghanistan, Kazakhstan, Turkmenistan, and Uzbekistan. M. c. concisa Thomas & Wroughton, 1907 — Algeria, Morocco, and Subsaharan Africa from Mauritania to Ethiopia. M.c. cotton: Lydekker, 1906 — C Africa from Gabon to Tanzania. M. M.c. inaurita Hodgson, 1836 — Nepal. \g M.c. indica Kerr, 1792 — India and Pakistan. M. M.c. maxwell Thomas, 1923 — Kenya and Somalia. \J M.c. pumalio Pocock, 1946 — S Arabian Peninsula and Yemen. M. M.c. signata Pocock, 1909 — Guinea and Sierra Leone. \f M.c. wilsoni Cheesman, 1920 — Iran, Iraq, Israel, Jordan, Kuwait, Lebanon, Saudi Arabia, and Syria. in Mustelidae
Subspecies and Distribution. M. c. capensis Schreber, 1776 — S Africa N to Angola, Mozambique, and Zambia. M. c. buechneri Baryshnikov, 2000 — C Asia including Afghanistan, Kazakhstan, Turkmenistan, and Uzbekistan. M. c. concisa Thomas & Wroughton, 1907 — Algeria, Morocco, and Subsaharan Africa from Mauritania to Ethiopia. M.c. cotton: Lydekker, 1906 — C Africa from Gabon to Tanzania. M. M.c. inaurita Hodgson, 1836 — Nepal. \g M.c. indica Kerr, 1792 — India and Pakistan. M. M.c. maxwell Thomas, 1923 — Kenya and Somalia. \J M.c. pumalio Pocock, 1946 — S Arabian Peninsula and Yemen. M. M.c. signata Pocock, 1909 — Guinea and Sierra Leone. \f M.c. wilsoni Cheesman, 1920 — Iran, Iraq, Israel, Jordan, Kuwait, Lebanon, Saudi Arabia, and Syria.
Fig. 3 in Streptomyces gossypiisoli sp. nov., isolated from cotton soil in Xinjiang, PR China
Fig. 3. Neighbour-joining phylogenetic tree based on concatenated partial sequences of the housekeeping genes atpD, gyrB, recA, rpoB and trpB. The relationships between strain TRM 44567T and the type strains of phylogenetically closely related species of the genus Streptomyces were analysed. *, Branches that were also found using the maximum-likelihood method; +, branches that were also found using the maximum-parsimony method; *+, branches that were found using all three methods. Numbers at nodes are percentage bootstrap values based on 1000 replicates; only values>50% are given. Bar, 0.0100 substitutions per nucleotide position.
Fig. 2 in Streptomyces gossypiisoli sp. nov., isolated from cotton soil in Xinjiang, PR China
Fig. 2. Neighbour-joining phylogenetic tree based on nearly complete 16S rRNA gene sequences. The relationships between strain TRM 44567T and the type strains of phylogenetically closely related species of the genus Streptomyces were analysed. Actinomadura hibisca JCM 9627T (AF163115) was used as the outgroup. *, Branches that were also found using the maximum- likelihood method; +, branches that were also found using the maximum-parsimony method; *+, branches that were found using all three methods. Numbers at nodes are percentage bootstrap values based on 1000 replicates; only values>50% are given. Bar, 0.0100 substitutions per nucleotide position.
Fig. 1 in Streptomyces gossypiisoli sp. nov., isolated from cotton soil in Xinjiang, PR China
Fig. 1. Scanning electron microscopy image of strain TRM 44567T grown on Gause's agar at 37 °C for 7 days. Bars, 5 µm (left) and 20 µm (right).
Cotton-based nucleic acid extraction
<p><strong>Abstract</strong>: Nucleic acid amplification technique (NAAT)-assisted detection is the primary intervention for pathogen molecular diagnostics. However, NAATs such as quantitative real-time polymerase chain reaction (qPCR) require prior purification or extraction of target nucleic acid from the sample of interest since the latter often contains polymerase inhibitors. Similarly, genetic disease screening is also reliant on the successful extraction of pure patient genomic DNA from the clinical sample. However, such extraction techniques traditionally utilize spin-column techniques that in turn require centralized high-speed centrifuges. This hinders any potential deployment of qPCR- or PCR-like NAAT methods in resource-constrained settings. The development of instrument-free nucleic acid extraction methods, especially those utilizing readily available materials would be of great interest and benefit to NAAT-mediated molecular diagnosis workflows in resource-constrained settings. In this report, we screened medical-grade cotton, a readily available over-the-counter biomaterial to extract <em>E. coli</em> genomic DNA (gDNA) spiked in 30%, 45%, and 60% serum. The extraction was carried out in a completely instrument-free manner using cotton and a sterilized toothpick and was completed in 30 min (with using chaotropic salt) or 10 min (without using chaotropic salt). The quality of the extracted DNA was then probed using PCR followed by agarose gel analysis, qPCR, and sequencing. Our method demonstrated that the high-quality DNA extraction could be performed both with or without using a chaotropic salt, albeit with a difference in the quality of the extracted DNA</p>
On following pages: 35. Cape Kudu (Strepsiceros strepsiceros); 36. Zambezi Kudu (Strepsiceros zambesiensis); 37. Northern Kudu (Strepsiceros chora); 38. Western Kudu (Strepsiceros cotton); 39. Common Eland (Taurotragus oryx); 40. Giant Eland (Taurotragus derbianus). in Bovidae
On following pages: 35. Cape Kudu (Strepsiceros strepsiceros); 36. Zambezi Kudu (Strepsiceros zambesiensis); 37. Northern Kudu (Strepsiceros chora); 38. Western Kudu (Strepsiceros cotton); 39. Common Eland (Taurotragus oryx); 40. Giant Eland (Taurotragus derbianus).
On following pages 34 Red-bel ıed Tarnann (Saguınus labıatusi 35 Emperor Tamann (Saguınus mpemron 36 Mıdas Tamann (Saguınus nudes) 37 Black-handed Tamann (Saguınııs nıgen 38 Pıed Tamann (Soguınus bıoolofi 39 Mamns s Bare-faced Tamann (Saguınus mamnsl) 40 Mottled-face Tırnann (Saguınus ınustusl 41 Whıte-fooıed Tamann (Saguınus Ieuoopus) 42 Cotton-top Tımann (Saguınus oedvøus). 43 Geoffroys Tamann (Saguınus gsafhoyñ in Callitrichiade
On following pages 34 Red-bel ıed Tarnann (Saguınus labıatusi 35 Emperor Tamann (Saguınus mpemron 36 Mıdas Tamann (Saguınus nudes) 37 Black-handed Tamann (Saguınııs nıgen 38 Pıed Tamann (Soguınus bıoolofi 39 Mamns s Bare-faced Tamann (Saguınus mamnsl) 40 Mottled-face Tırnann (Saguınus ınustusl 41 Whıte-fooıed Tamann (Saguınus Ieuoopus) 42 Cotton-top Tımann (Saguınus oedvøus). 43 Geoffroys Tamann (Saguınus gsafhoyñ
On following pages: 325. Tawny-bellied Cotton Rat (Sigmodon fulviventer); 326. Yellow-nosed Cotton Rat (Sigmodon ochrognathus); 327. Hispid Cotton Rat (Sigmodon hispidus); 328. West Mexican Cotton Rat (Sigmodon mascotensis); 329. Arizona Cotton Rat (Sigmodon arizonae); 330. Toltec Cotton Rat (Sigmodon toltecus); 331. Allen's Cotton Rat (Sigmodon alleni); 332. Burmeister's Cotton Rat (Sigmodon hirsutus); 333. Montane Cotton Rat (Sigmodon zanjonensis); 334. Miahuatlan Cotton Rat (Sigmodon planifrons); 335. Musso's Fish-eating Rat (Neusticomys mussol); 336. Montane Fish-eating Rat (Neusticomys monticolus); 337 Voss's Fish-eating Rat (Neusticomys vossi); 338. Venezuelan Fish-eating Rat (Neusticomys venezuelae); 339. Guianan Fish-eating Rat (Neusticomys oyapocki); 340. Ferreira's Fish-eating Rat (Neusticomys ferreirai); 341. Peruvian Fish-eating Rat (Neusticomys peruviensis); 342. Northern Andean Water Mouse (Chibchanomys trichotis); 343. Orces's Andean Water Mouse (Chibchanomys orcesi); 344. Earless Water Mouse (Anotomys leander); 345. Pittier's Crab-eating Rat (/chthyomys pittieri); 346. Common Crab-eating Rat (/chthyomys hydrobates); 347 Tweedy's Crab-eating Rat (/chthyomys tweed); 348. Stolzmann''s Crab-eating Rat (/chthyomys stolzmanni); 349. Goldman's Water Mouse (Rheomys raptor); 350. Thomas's Water Mouse (Rheomys thomasi); 351. Underwood's Water Mouse (Rheomys underwood); 352. Mexican Water Mouse (Rheomys mexicanus). in Cricetidae
On following pages: 325. Tawny-bellied Cotton Rat (Sigmodon fulviventer); 326. Yellow-nosed Cotton Rat (Sigmodon ochrognathus); 327. Hispid Cotton Rat (Sigmodon hispidus); 328. West Mexican Cotton Rat (Sigmodon mascotensis); 329. Arizona Cotton Rat (Sigmodon arizonae); 330. Toltec Cotton Rat (Sigmodon toltecus); 331. Allen's Cotton Rat (Sigmodon alleni); 332. Burmeister's Cotton Rat (Sigmodon hirsutus); 333. Montane Cotton Rat (Sigmodon zanjonensis); 334. Miahuatlan Cotton Rat (Sigmodon planifrons); 335. Musso's Fish-eating Rat (Neusticomys mussol); 336. Montane Fish-eating Rat (Neusticomys monticolus); 337 Voss's Fish-eating Rat (Neusticomys vossi); 338. Venezuelan Fish-eating Rat (Neusticomys venezuelae); 339. Guianan Fish-eating Rat (Neusticomys oyapocki); 340. Ferreira's Fish-eating Rat (Neusticomys ferreirai); 341. Peruvian Fish-eating Rat (Neusticomys peruviensis); 342. Northern Andean Water Mouse (Chibchanomys trichotis); 343. Orces's Andean Water Mouse (Chibchanomys orcesi); 344. Earless Water Mouse (Anotomys leander); 345. Pittier's Crab-eating Rat (/chthyomys pittieri); 346. Common Crab-eating Rat (/chthyomys hydrobates); 347 Tweedy's Crab-eating Rat (/chthyomys tweed); 348. Stolzmann''s Crab-eating Rat (/chthyomys stolzmanni); 349. Goldman's Water Mouse (Rheomys raptor); 350. Thomas's Water Mouse (Rheomys thomasi); 351. Underwood's Water Mouse (Rheomys underwood); 352. Mexican Water Mouse (Rheomys mexicanus).
On following pages: 248. Merriam''s Deermouse (Peromyscus merriami); 249. Cactus Deermouse (Peromyscus eremicus); 250. San Lorenzo Deermouse (Peromyscus interparietalis); 251. Southern Baja Deermouse (Peromyscus eva); 252. Northern Baja Deermouse (Peromyscus fraterculus); 253. Monserrat Island Deermouse (Peromyscus caniceps); 254. Dickey's Deermouse (Peromyscus dickeyi); 255. La Guarda Deermouse (Peromyscus guardia); 256. Coronados Deermouse (Peromyscus pseudocrinitus); 257. Cotton Deermouse (Peromyscus gossypinus); 258. White-footed Deermouse (Peromyscus leucopus); 259. Santa Cruz Deermouse (Peromyscus sejugis); 260. North-western Deermouse (Peromyscus keeni): 261. Oldfield Deermouse (Peromyscus polionotus); 262. North American Deermouse (Peromyscus maniculatus); 263. Black-eared Deermouse (Peromyscus melanotis); 264. Black-tailed Deermouse (Peromyscus melanurus); 265. Broad-faced Deermouse (Peromyscus megalops); 266. Black-wristed Deermouse (Peromyscus melanocarpus); 267. Catalina Deermouse (Peromyscus slevini); 268. Tawny Deermouse (Peromyscus perfulvus); 269. Plateau Deermouse (Peromyscus melanophrys); 270. Puebla Deermouse (Peromyscus mekisturus); 271. Mayan Deermouse (Peromyscus mayensis); 272. Stirton's Deermouse (Peromyscus stirtoni); 273. Yucatan Deermouse (Peromyscus yucatanicus); 274. Chimoxan Deermouse (Peromyscus tropicalis); 275. Talamancan Deermouse (Peromyscus nudipes); 276. Mexican Deermouse (Peromyscus mexicanus); 277. Naked-eared Deermouse (Peromyscus gymnotis); 278. Chiapan Deermouse (Peromyscus zarhynchus); 279. Gardner's Deermouse (Peromyscus gardneri); 280. Nicaraguan Deermouse (Peromyscus nicaraguae); 281. Salvadorean Deermouse (Peromyscus salvadorensis); 282. Guatemalan Deermouse (Peromyscus guatemalensis); 283. Large Deermouse (Peromyscus grandis). in Cricetidae
On following pages: 248. Merriam''s Deermouse (Peromyscus merriami); 249. Cactus Deermouse (Peromyscus eremicus); 250. San Lorenzo Deermouse (Peromyscus interparietalis); 251. Southern Baja Deermouse (Peromyscus eva); 252. Northern Baja Deermouse (Peromyscus fraterculus); 253. Monserrat Island Deermouse (Peromyscus caniceps); 254. Dickey's Deermouse (Peromyscus dickeyi); 255. La Guarda Deermouse (Peromyscus guardia); 256. Coronados Deermouse (Peromyscus pseudocrinitus); 257. Cotton Deermouse (Peromyscus gossypinus); 258. White-footed Deermouse (Peromyscus leucopus); 259. Santa Cruz Deermouse (Peromyscus sejugis); 260. North-western Deermouse (Peromyscus keeni): 261. Oldfield Deermouse (Peromyscus polionotus); 262. North American Deermouse (Peromyscus maniculatus); 263. Black-eared Deermouse (Peromyscus melanotis); 264. Black-tailed Deermouse (Peromyscus melanurus); 265. Broad-faced Deermouse (Peromyscus megalops); 266. Black-wristed Deermouse (Peromyscus melanocarpus); 267. Catalina Deermouse (Peromyscus slevini); 268. Tawny Deermouse (Peromyscus perfulvus); 269. Plateau Deermouse (Peromyscus melanophrys); 270. Puebla Deermouse (Peromyscus mekisturus); 271. Mayan Deermouse (Peromyscus mayensis); 272. Stirton's Deermouse (Peromyscus stirtoni); 273. Yucatan Deermouse (Peromyscus yucatanicus); 274. Chimoxan Deermouse (Peromyscus tropicalis); 275. Talamancan Deermouse (Peromyscus nudipes); 276. Mexican Deermouse (Peromyscus mexicanus); 277. Naked-eared Deermouse (Peromyscus gymnotis); 278. Chiapan Deermouse (Peromyscus zarhynchus); 279. Gardner's Deermouse (Peromyscus gardneri); 280. Nicaraguan Deermouse (Peromyscus nicaraguae); 281. Salvadorean Deermouse (Peromyscus salvadorensis); 282. Guatemalan Deermouse (Peromyscus guatemalensis); 283. Large Deermouse (Peromyscus grandis).
FIGURES 37–40 in Review of Chinese species of the leafhopper genus Amrasca Ghauri (Hemiptera, Cicadellidae, Typhlocybinae), with description of a new species, species checklist and notes on the identity of the Indian cotton leafhopper
FIGURES 37–40. Amrasca (Quartasca) czerwcowa (Dworakowska). 37. male adult (abdomen removed), dorsal view; 38. male adult (abdomen removed), left lateral view; 39. head and thorax, dorsal view; 40. face. Scale bars = 0.5 mm (Figs 37, 38), 0.2 mm (Figs 39, 40).
FIGURES 18–26 in Review of Chinese species of the leafhopper genus Amrasca Ghauri (Hemiptera, Cicadellidae, Typhlocybinae), with description of a new species, species checklist and notes on the identity of the Indian cotton leafhopper
FIGURES 18–26. Amrasca (Amrasca) complana Qin, Wang & Xu, sp. nov. 18. male adult (abdomen removed), dorsal view; 19. head and thorax, dorsal view; 20. face; 21. head and thorax, left lateral view; 22. forewing; 23. hind wing; 24. abdominal apodemes; 25. male genitalia, dorsal view; 26. male genitalia, left lateral view. Scale bars = 0.5 mm (Figs 18, 22, 23), 0.2 mm (Figs 19–21, 24); 0.1 mm (Figs 25, 26).
FIGURES 6–17 in Review of Chinese species of the leafhopper genus Amrasca Ghauri (Hemiptera, Cicadellidae, Typhlocybinae), with description of a new species, species checklist and notes on the identity of the Indian cotton leafhopper
FIGURES 6–17: 6–9. Amrasca (Amrasca) splendens Ghauri; 10–13. Amrasca (Amrasca) bombaxia (Ghauri); 14–17. Amrasca (Amrasca) uvka Dworakowska. 6, 10, 14. adult, dorsal view; 7, 11, 15. adult, left lateral view; 8, 12, 16. head and thorax, dorsal view; 9, 13, 17. face. Scale bars = 0.5 mm (Figs 6, 7, 10, 11, 14, 15), 0.2 mm (Figs 8, 9, 12, 13, 16, 17).
FIGURES 1–5 in Review of Chinese species of the leafhopper genus Amrasca Ghauri (Hemiptera, Cicadellidae, Typhlocybinae), with description of a new species, species checklist and notes on the identity of the Indian cotton leafhopper
FIGURES 1–5. Amrasca (Sundapteryx) biguttula (Ishida). 1. adult, dorsal view; 2. adult, left lateral view; 3. head and thorax, dorsal view; 4. face; 5. male abdomen and male genitalia, dorsal view. Scale bars = 0.5 mm (Figs 1, 2), 0.2 mm (Figs 3, 4).
FIGURES 27–36 in Review of Chinese species of the leafhopper genus Amrasca Ghauri (Hemiptera, Cicadellidae, Typhlocybinae), with description of a new species, species checklist and notes on the identity of the Indian cotton leafhopper
FIGURES 27–36. Amrasca (Amrasca) complana Qin, Wang & Xu, sp. nov. 27. male genitalia, left lateral view; 28. pygofer side and ventral pygofer appendage, left lateral view; 29. pygofer side, dorsal view; 30. ventral pygofer appendage; 31. aedeagus, left lateral view; 32. aedeagus, ventral view; 33. connective; 34. subgenital plate; 35. paramere; 36. anal tube, left lateral view. Scale bars = 0.1 mm (Figs 27–36).
Figure 1 in In Memoriam From Cotton Farming to the Congressional Gold Medal: The Career and Legacy of Ernest James Harris (1928-2018)
Figure 1: A–B: Ernie Harris ca. 1929 and in the early 1950s. C: Ernie and Betty Jo Harris and children Mark and Tanya arriving at the Honolulu Airport in February 1962. D: Early prototype of the Jackson trap, scanned from Ernie's private slide collection, photo dated June 1968. E: Last meeting between Ernie and the authors in March 2017.
The pan-gene, pan-genome, and SV-eQTL dataset for A2 and AD1 cotton.
Open the record for dataset details and reuse information.
Plant-to-plant defence induction in cotton is mediated by delayed release of volatiles upon herbivory
<p>Data and R scripts for statistical analyses for the article <strong>"Plant-to-plant defence induction in cotton is mediated by delayed release of volatiles upon herbivory"</strong>.</p> <p>By: Luca Grandi, Wenfeng Ye, Mary V. Clancy, Armelle Vallat, Gaétan Glauser, Luis Abdala-Roberts, Thierry Brevault, Betty Benrey, Ted C.J. Turlings, Carlos Bustos-Segura</p> <p><strong>Summary:</strong></p> <p>· Caterpillar feeding immediately triggers the release of volatile compounds stored in the leaves of cotton plants. Additionally, after one day of herbivory, the leaves release other newly synthesised volatiles. We investigated whether these volatiles affect chemical defences in neighbouring plants and whether such temporal shifts in emissions matter for signalling between plants. </p> <p>· Undamaged receiver plants were exposed to volatiles from plants infested with <em>Spodoptera </em>caterpillars. For receiver plants, we measured changes in defence-related traits such as volatile emissions, secondary metabolites, phytohormones, gene expression, and caterpillar feeding preference. Then, we compared the effects of volatiles emitted prior to and after 24 h of damage on neighbouring plant defences. </p> <p>· Genes that were upregulated in receiver plants following exposure to volatiles from damaged plants were the same as those activated directly by herbivory on a plant. Only volatiles emitted after 24 h of damage, including newly produced volatiles, were found to increase phytohormone levels, upregulate defence genes, and enhance resistance to caterpillars.</p> <p>· These results indicate that the defence induction by volatiles is a specific response to <em>de novo</em> synthesised volatiles, suggesting that these compounds are honest signals of herbivore attack. These findings point to an adaptive origin of airborne signalling between plants.</p>
Figure 1 in Natural occurrence of entomopathogenic nematode species (Rhabditida: Steinernematidae and Heterorhabditidae) in cotton fields of Tamil Nadu, India
Figure 1. Geographic regions of Tamil Nadu state of india showing sampling sites. 1. Villupuram District; 2. Erode District; 3. Coimbatore District; 4. Ariyalur District; 5. Dindigul District; 6. Theni District; 7. Madurai District; 8. Virudhunagar District; 9. Thirunelveli District; 10. Thoothukudi District. Positive sampling sites: Steinernema carpocapsae, filled square; Steinernema siamkayai, filled triangle; Steinernema monticolum, filled circle; Heterorhabditis bacteriophora, filled star. Negative sampling site, open circle.
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