Find research datasets worth reusing
Search datasets from major research repositories and use ShareScore to quickly assess how well each record supports discovery, access, and reuse.
1,003
datasets available to search
ShareScore release 0.9.0
Dataset results
1,003 results for “darkness”
Dark Hill Mine Shaft
Mine shaft at Dark Hill Iron Works, Forest of Dean Created with Polycam and iPhone 12 Pro Max Source: Objaverse 1.0 / Sketchfab
Figure 3. Xianguangia sinica with dark patches. A–C, YNGIP 90001, A, a in Tentacular nature of the 'column' of the Cambrian diploblastic Xianguangia sinica
Figure 3. Xianguangia sinica with dark patches. A–C, YNGIP 90001, A, a complete specimen in lateral view showing a pair of dark patches preserved in the lower central region of the 'column'; B, a close-up image of the dark patch region; C, a fluorescent image showing the patches likely originated from the oral surface. D, YNGIP 90002a, a close-up image showing three dark patches. E, YNGIP 90003, a close-up of the dark patch region, showing two lateral patches inclined towards the middle one. Abbreviations: Ca, cavity; Cal, calyx; Dp, dark patch; Ds, dark stain; Mo, mouth; Pin, pinnule. Scale bars: A, D, E = 2 mm; B, C = 1 mm.
Figure files and simulation code for The formation of a nuclear-spin dark state in silicon
<p>This repository contains MATLAB figure files and simulation code for The formation of a nuclear-spin dark state in silicon. It includes a Readme file that provides a brief description of each file's contents.</p>
A Comprehensive Study on Dark Patterns
<p>It concludes the data of Three research questions. </p> <p>Data of RQ1: taxonomy.xlsx</p> <p>Data of RQ2:InfoOftools.xlsx/CoverageOfTools.xlsx</p> <p>Data of RQ3:InfoOfDatasets.xlsx/CoverageOfDatasets.xlsx</p>
Supplementary Data: A global fit of non-relativistic effective dark matter operators including solar neutrinos
<p>The files within contain the data from <a href="https://gambitbsm.org/">GAMBIT</a> scans and the scripts to recreate the plots in Avis Kozar et al. "A global fit of non-relativistic effective dark matter operators including solar neutrinos" using <a href="https://www.python.org/">Python</a> and <a href="https://github.com/GambitBSM/pippi">pippi</a>.</p>
Experimental source data for "A photosensitiser-polyoxometalate dyad that enables the decoupling of light- and dark-reactions for delayed on-demand solar hydrogen production"
<p>Experimental data for the manuscript "A photosensitiser-polyoxometalate dyad that enables the decoupling of light- and dark-reactions for delayed on-demand solar hydrogen production"</p>
Distribution. Angola, DR Congo, Malawi, Mozambique, Tanzania, and Zambia. Description. Head-body 46:5-47-8 cm (males), 44-45-5 cm (females), tail 40-43 cm (males), 38-39 cm (females), hindfoot 8:7-9-8 cm (males), 8-9 cm (females), ear 4-7-5-4 cm (males), 5-1-5-8 cm (females); weight 1-3-2 kg. The coat color is pale ocher, with brownish or grayish tones; melanistic individuals are quite common. The throat and chest are blackish, and the ventral pelage varies from creamy white to dirty white. The stripes and spots on the body vary from different hues of brown to black. The nuchal stripes run as two parallel lines from the nape to the shoulders, where they diverge and enlarge towards the elbows; they are not so conspicuously marked as in other genet species. Below them, a pair of thinner stripes and small spots are scattered on the shoulders and sides of the neck. A third pair of thinner, parallel stripes runs down the neck between the nuchal stripes, extending to about one fourth of the mid-dorsal line, where they vanish or diverge as the first row of flank spots. The black mid-dorsal line is continuous and is flanked on each side by four rows of oblong to squared spots, and by a few small-scattered spots below. There is a dorsal erectile crest. The face has a dark mask and a pair of white sub-ocular spots. The tail has seven to nine black rings, alternating with pale rings; the intervening white spaces are pigmented with a brownish tinge on the dorsal midline. The width of the pale rings relative to the dark rings in the middle of the tail is 50-75%; the tip of the tail is dark. The hindlimbs and forelimbs are black; there are white hairs on the metacarpals and metatarsals. [he posterior parts of the feet are dark. There are two pairs of teats. The posterior chamber of the auditory bulla is not ventrally inflated and has a continuous curve line on the external side. The ratio between the inter-orbital constriction and frontal width is 1-00 + 0-12. Dental formula: 13/3, C1/1,P 4/4, M 2/2 = 40. in Viverridae
Distribution. Angola, DR Congo, Malawi, Mozambique, Tanzania, and Zambia. Description. Head-body 46:5-47-8 cm (males), 44-45-5 cm (females), tail 40-43 cm (males), 38-39 cm (females), hindfoot 8:7-9-8 cm (males), 8-9 cm (females), ear 4-7-5-4 cm (males), 5-1-5-8 cm (females); weight 1-3-2 kg. The coat color is pale ocher, with brownish or grayish tones; melanistic individuals are quite common. The throat and chest are blackish, and the ventral pelage varies from creamy white to dirty white. The stripes and spots on the body vary from different hues of brown to black. The nuchal stripes run as two parallel lines from the nape to the shoulders, where they diverge and enlarge towards the elbows; they are not so conspicuously marked as in other genet species. Below them, a pair of thinner stripes and small spots are scattered on the shoulders and sides of the neck. A third pair of thinner, parallel stripes runs down the neck between the nuchal stripes, extending to about one fourth of the mid-dorsal line, where they vanish or diverge as the first row of flank spots. The black mid-dorsal line is continuous and is flanked on each side by four rows of oblong to squared spots, and by a few small-scattered spots below. There is a dorsal erectile crest. The face has a dark mask and a pair of white sub-ocular spots. The tail has seven to nine black rings, alternating with pale rings; the intervening white spaces are pigmented with a brownish tinge on the dorsal midline. The width of the pale rings relative to the dark rings in the middle of the tail is 50-75%; the tip of the tail is dark. The hindlimbs and forelimbs are black; there are white hairs on the metacarpals and metatarsals. [he posterior parts of the feet are dark. There are two pairs of teats. The posterior chamber of the auditory bulla is not ventrally inflated and has a continuous curve line on the external side. The ratio between the inter-orbital constriction and frontal width is 1-00 + 0-12. Dental formula: 13/3, C1/1,P 4/4, M 2/2 = 40.
Colour illustrations. Flowers, fruits, leaves and seeds of Musa itinerans (background photo by D.T. Vu); from top to bottom and left to right: colony on PDA after 14 d at 24 °C in darkness (left = obverse,right = reverse), sporodochia formed on CLA, aerial conidiophore, aerial conidiogenous cells, aerial conidia, sporodochial conidia. Scale bars: black = 20 µm, white = 10 µm. in Fusarium chuoi R. Hill, Gaya, D.T. Vu, Sand.-Den. & Crous, R. Hill, Gaya, D.T. Vu, Sand.-Den. & Crous sp. nov.
Colour illustrations. Flowers, fruits, leaves and seeds of Musa itinerans (background photo by D.T. Vu); from top to bottom and left to right: colony on PDA after 14 d at 24 °C in darkness (left = obverse,right = reverse), sporodochia formed on CLA, aerial conidiophore, aerial conidiogenous cells, aerial conidia, sporodochial conidia. Scale bars: black = 20 µm, white = 10 µm.
Data for SWATH-based Quantitative Proteomic Analysis of Morus alba L. Leaf under Ultraviolet-B radiation and Dark Treatment
<p><em>Morus alba (M. alba) </em>have been used in traditional Chinese medicine. Since, previous studies indicated that the accumulation of several secondary metabolites was significantly induced by UV-B radiation with dark treatment. To investigate the response of <em>Morus alba</em> leaf to UV-B radiation and UV-B radiation followed by dark incubation (UVD), SWATH-based quantitative proteomic analysis was performed on <em>Morus alba</em> leaf of control, UV-B radiation and UV-B radiation then dark incubation. A total of 716 proteins were identified and quantified.</p>
The 'dark matter' of protein variants carries a distinct DNA signature and predicts damaging variant effects
<p>Data generated for the manuscript "The 'dark matter' of protein variants carries a distinct DNA signature and predicts damaging variant effects".</p> <p> </p> <p>Please consult the README file for detailed description of data files included in this dataset.</p>
FIGURE 7. Mahechadendron puntecascarillo. A. Tree recently cut down. B. Tree stump showing the dark heartwood. C in Mahechadendron puntecascarillo (Vochysiaceae), a new genus and forest tree species from Colombia
FIGURE 7. Mahechadendron puntecascarillo. A. Tree recently cut down. B. Tree stump showing the dark heartwood. C. Sawn timber in the field. Photos by W. Ariza-Cortés.
On following pages: 368. Himalayan Broad-muzzled Bat (Submyotodon caliginosus); 369. Moupin Broad-muzzled Bat (Submyotodon moupinensis); 370. Northern Myotis (Myotis septentrionalis); 371. South-western Myotis (Myotis auriculus); 372. Western Small-footed Myotis (Myotis ciliolabrum); 373. Dark-nosed Small-footed Myotis (Myotis melanorhinus); 374. Eastern Small-footed Myotis (Myotis leibil); 375. California Myotis (Myotis californicus); 376. Little Brown Myotis (Myotis lucifugus); 377. Keen's Myotis (Myotis keenii); 378. Long-eared Myotis (Myotis evotis); 379. Fringed Myotis (Myotis thysanodes); 380. Arizona Myotis (Myotis occultus); 381. Longlegged Myotis (Myotis volans); 382. Flat-headed Myotis (Myotis planiceps); 383. Indiana Myotis (Myotis sodalis); 384. Cinnamon Myotis (Myotis fortidens); 385. Findley's Myotis (Myotis findley)); 386. Northern Hairy-legged Myotis (Myotis pilosatibialis); 387. Southern Hairy-legged Myotis (Myotis keaysi); 388. Red Myotis (Myotis ruber); 389. Riparian Myotis (Myotis riparius); 390. Velvety Myotis (Myotis simus); 391. Golden Myotis (Myotis midastactus); 392. Elegant Myotis (Myotis elegans); 393. Fish-eating Myotis (Myotis vives). in Vespertilionidae
On following pages: 368. Himalayan Broad-muzzled Bat (Submyotodon caliginosus); 369. Moupin Broad-muzzled Bat (Submyotodon moupinensis); 370. Northern Myotis (Myotis septentrionalis); 371. South-western Myotis (Myotis auriculus); 372. Western Small-footed Myotis (Myotis ciliolabrum); 373. Dark-nosed Small-footed Myotis (Myotis melanorhinus); 374. Eastern Small-footed Myotis (Myotis leibil); 375. California Myotis (Myotis californicus); 376. Little Brown Myotis (Myotis lucifugus); 377. Keen's Myotis (Myotis keenii); 378. Long-eared Myotis (Myotis evotis); 379. Fringed Myotis (Myotis thysanodes); 380. Arizona Myotis (Myotis occultus); 381. Longlegged Myotis (Myotis volans); 382. Flat-headed Myotis (Myotis planiceps); 383. Indiana Myotis (Myotis sodalis); 384. Cinnamon Myotis (Myotis fortidens); 385. Findley's Myotis (Myotis findley)); 386. Northern Hairy-legged Myotis (Myotis pilosatibialis); 387. Southern Hairy-legged Myotis (Myotis keaysi); 388. Red Myotis (Myotis ruber); 389. Riparian Myotis (Myotis riparius); 390. Velvety Myotis (Myotis simus); 391. Golden Myotis (Myotis midastactus); 392. Elegant Myotis (Myotis elegans); 393. Fish-eating Myotis (Myotis vives).
On following pages: 121. Roberts's Serotine (Neoromicia robertsi); 122. Stanley's Serotine (Neoromicia stanleyi); 123. Zulu Serotine (Neoromicia zuluensis): 124. Tiny Serotine (Neoromicia guineensis); 125. Somali Serotine (Neoromicia somalica); 126. Banana Serotine (Neoromicia nanus); 127. Rendall''s Serotine (Neoromicia rendall): 128. Dark-brown Serotine (Neoromicia brunnea); 129. Rosevear's Serotine (Neoromicia rosevear): 130. Isabelline Serotine (Neoromicia isabella); 131. Grandidier's Serotine (Neoromicia grandidieri); 132. White-winged Serotine (Neoromicia tenuipinnis); 133. Heller's Serotine (Neoromicia helios); 134. De Winton's Long-eared Bat (Laephotis wintoni); 135. Angolan Long-eared Bat (Laephotis angolensis); 136. Botswanan Long-eared Bat (Laephotis botswanae); 137. Namib Long-eared Bat (Laephotis namibensis): 138. Sind Bat (Rhyneptesicus nasutus); 139. Collared Sprite (Thainycteris aureocollaris); 140. Necklace Sprite (Thainycteris torquatus); 141. Bronze Sprite (Arielulus circumdatus); 142. Social Sprite (Arielulus societatis); 143. Coppery Sprite (Arielulus cuprosus). in Vespertilionidae
On following pages: 121. Roberts's Serotine (Neoromicia robertsi); 122. Stanley's Serotine (Neoromicia stanleyi); 123. Zulu Serotine (Neoromicia zuluensis): 124. Tiny Serotine (Neoromicia guineensis); 125. Somali Serotine (Neoromicia somalica); 126. Banana Serotine (Neoromicia nanus); 127. Rendall''s Serotine (Neoromicia rendall): 128. Dark-brown Serotine (Neoromicia brunnea); 129. Rosevear's Serotine (Neoromicia rosevear): 130. Isabelline Serotine (Neoromicia isabella); 131. Grandidier's Serotine (Neoromicia grandidieri); 132. White-winged Serotine (Neoromicia tenuipinnis); 133. Heller's Serotine (Neoromicia helios); 134. De Winton's Long-eared Bat (Laephotis wintoni); 135. Angolan Long-eared Bat (Laephotis angolensis); 136. Botswanan Long-eared Bat (Laephotis botswanae); 137. Namib Long-eared Bat (Laephotis namibensis): 138. Sind Bat (Rhyneptesicus nasutus); 139. Collared Sprite (Thainycteris aureocollaris); 140. Necklace Sprite (Thainycteris torquatus); 141. Bronze Sprite (Arielulus circumdatus); 142. Social Sprite (Arielulus societatis); 143. Coppery Sprite (Arielulus cuprosus).
On following pages: 296. Golden-tipped Bat (Phoniscus papuensis); 297. Hardwicke's Woolly Bat (Kerivoula hardwickii); 298. Flat-skulled Woolly Bat (Kerivoula depressa); 299. Sri Lankan Woolly Bat (Kerivoula malpasi: 300. Cryptic Woolly Bat (Kerivoula crypta); 301. Dark Woolly Bat (Kerivoula furva); 302. Kachin Woolly Bat (Kerivoula kachinensis); 303. Indochinese Woolly Bat (Kerivoula dongduongana); 304. Krau Woolly Bat (Kerivoula krauensis); 305. Titania's Woolly Bat (Kerivoula titania); 306. Least Woolly Bat (Kerivoula minuta); 307. Small Woolly Bat (Kerivoula intermedia); 308. Papillose Woolly Bat (Kerivoula papillosa); 309. Lenis Woolly Bat (Kerivoula lenis); 310. Clearwinged Woolly Bat (Kerivoula pellucida); 311. Painted Woolly Bat (Kerivoula picta); 312. Whitehead's Woolly Bat (Kerivoula whitehead); 313. Flores Woolly Bat (Kerivoula flora); 314. Fly River Woolly Bat (Kerivoula muscina); 315. Saint Aignan's Woolly Bat (Kerivoula agnella); 316. Bismarck Woolly Bat (Kerivoula myrella); 317. Lesser Woolly Bat (Kerivoula lanosa); 318. Ethiopian Woolly Bat (Kerivoula eriophora); 319. Tanzanian Woolly Bat Kerivoula africana); 320. Smith's Woolly Bat (Kerivoula smithii); 321. Coppery Woolly Bat (Kerivoula cuprosa); 322. Spurrell's Woolly Bat (Kerivoula phalaena); 323. Damara Woolly Bat (Kerivoula argentata). in Vespertilionidae
On following pages: 296. Golden-tipped Bat (Phoniscus papuensis); 297. Hardwicke's Woolly Bat (Kerivoula hardwickii); 298. Flat-skulled Woolly Bat (Kerivoula depressa); 299. Sri Lankan Woolly Bat (Kerivoula malpasi: 300. Cryptic Woolly Bat (Kerivoula crypta); 301. Dark Woolly Bat (Kerivoula furva); 302. Kachin Woolly Bat (Kerivoula kachinensis); 303. Indochinese Woolly Bat (Kerivoula dongduongana); 304. Krau Woolly Bat (Kerivoula krauensis); 305. Titania's Woolly Bat (Kerivoula titania); 306. Least Woolly Bat (Kerivoula minuta); 307. Small Woolly Bat (Kerivoula intermedia); 308. Papillose Woolly Bat (Kerivoula papillosa); 309. Lenis Woolly Bat (Kerivoula lenis); 310. Clearwinged Woolly Bat (Kerivoula pellucida); 311. Painted Woolly Bat (Kerivoula picta); 312. Whitehead's Woolly Bat (Kerivoula whitehead); 313. Flores Woolly Bat (Kerivoula flora); 314. Fly River Woolly Bat (Kerivoula muscina); 315. Saint Aignan's Woolly Bat (Kerivoula agnella); 316. Bismarck Woolly Bat (Kerivoula myrella); 317. Lesser Woolly Bat (Kerivoula lanosa); 318. Ethiopian Woolly Bat (Kerivoula eriophora); 319. Tanzanian Woolly Bat Kerivoula africana); 320. Smith's Woolly Bat (Kerivoula smithii); 321. Coppery Woolly Bat (Kerivoula cuprosa); 322. Spurrell's Woolly Bat (Kerivoula phalaena); 323. Damara Woolly Bat (Kerivoula argentata).
On following pages: 190. Hairy Fruit-eating Bat (Artibeus hirsutus); 191. Fringed Fruit-eating Bat (Artibeus fimbriatus); 192. Ecuadorian Fruit-eating Bat (Artibeus aequatorialis); 193. Jamaican Fruit-eating Bat (Artibeus jamaicensis); 194. Dark Fruit-eating Bat (Artibeus obscurus); 195. Schwartz's Fruit-eating Bat (Artibeus schwartz); 196. Great Fruit-eating Bat (Artibeus lituratus); 197. Large Fruit-eating Bat (Artibeus amplus); 198. Flat-faced Fruit-eating Bat (Artibeus planirostris); 199. Rosenberg's Fruit-eating Bat (Artibeus rosenbergi); 200. Thomas's Fruit-eating Bat (Artibeus watson); 201. Toltec Fruit-eating Bat (Artibeus toltecus); 202. Pygmy Fruit-eating Bat (Artibeus phaeotis); 203. Gervais's Fruit-eating Bat (Artibeus cinereus); 204. Andersen's Fruit-eating Bat (Artibeus anderseni); 205. Little Fruit-eating Bat (Artibeusravus); 206. Aztec Fruit-eating Bat (Artibeus aztecus); 207. Bogota Fruit-eating Bat (Artibeus bogotensis); 208. Silvery Fruit-eating Bat (Artibeus glaucus); 209. Dwarf Fruit-eating Bat (Artibeus gnomus); 210. Jamaican Fig-eating Bat (Ariteus flavescens); 211. Tree Bat (Ardops nicholls); 212. Red Fruit Bat (Stenoderma rufum); 213. Wrinkle-faced Bat (Centurio senex): 214. Ipanema Broad-nosed Bat (Pygoderma bilabiatum); 215. Visored Bat (Sphaeronycteris toxophyllum); 216. Little White-shouldered Bat (Ametrida centurio); 217. Cuban Fig-eating Bat (Phyllops falcatus). in Phyllostomidae
On following pages: 190. Hairy Fruit-eating Bat (Artibeus hirsutus); 191. Fringed Fruit-eating Bat (Artibeus fimbriatus); 192. Ecuadorian Fruit-eating Bat (Artibeus aequatorialis); 193. Jamaican Fruit-eating Bat (Artibeus jamaicensis); 194. Dark Fruit-eating Bat (Artibeus obscurus); 195. Schwartz's Fruit-eating Bat (Artibeus schwartz); 196. Great Fruit-eating Bat (Artibeus lituratus); 197. Large Fruit-eating Bat (Artibeus amplus); 198. Flat-faced Fruit-eating Bat (Artibeus planirostris); 199. Rosenberg's Fruit-eating Bat (Artibeus rosenbergi); 200. Thomas's Fruit-eating Bat (Artibeus watson); 201. Toltec Fruit-eating Bat (Artibeus toltecus); 202. Pygmy Fruit-eating Bat (Artibeus phaeotis); 203. Gervais's Fruit-eating Bat (Artibeus cinereus); 204. Andersen's Fruit-eating Bat (Artibeus anderseni); 205. Little Fruit-eating Bat (Artibeusravus); 206. Aztec Fruit-eating Bat (Artibeus aztecus); 207. Bogota Fruit-eating Bat (Artibeus bogotensis); 208. Silvery Fruit-eating Bat (Artibeus glaucus); 209. Dwarf Fruit-eating Bat (Artibeus gnomus); 210. Jamaican Fig-eating Bat (Ariteus flavescens); 211. Tree Bat (Ardops nicholls); 212. Red Fruit Bat (Stenoderma rufum); 213. Wrinkle-faced Bat (Centurio senex): 214. Ipanema Broad-nosed Bat (Pygoderma bilabiatum); 215. Visored Bat (Sphaeronycteris toxophyllum); 216. Little White-shouldered Bat (Ametrida centurio); 217. Cuban Fig-eating Bat (Phyllops falcatus).
Data for: Dark matters – contrasting responses of stream biofilm to browning and loss of riparian shading
<p><span>Concentrations of terrestrial-derived dissolved organic carbon (DOC) in freshwater ecosystems have increased consistently, causing freshwater browning. The mechanisms behind browning are complex, but in forestry-intensive regions browning is accelerated by land drainage. Forestry actions in streamside riparian forests alter canopy shading, which together with browning is expected to exert a complex and largely unpredictable control over key ecosystem functions. We conducted a stream mesocosm experiment with three levels of browning (ambient vs. moderate vs. high, with 2.7 and 5.5-fold increase, respectively, in absorbance) crossed with two levels of riparian shading (70% light reduction vs. open canopy) to explore the individual and combined effects of browning and loss of shading on the quantity (algal biomass) and nutritional quality (polyunsaturated fatty acid and sterol content) of the periphytic biofilm. We also conducted a field survey of differently colored (4.7 to 26.2 mg DOC L<sup>-1</sup>) streams to provide a 'reality check' for our experimental findings. Browning reduced greatly the algal biomass, suppressed the availability of essential polyunsaturated fatty acids, especially eicosapentaenoic acid (EPA), and sterols, but increased the availability of terrestrial-derived long-chain saturated fatty acids (LSAFA). In contrast, loss of shading increased primary productivity, which resulted in elevated sterol and EPA content of the biofilm. The field survey largely repeated the same pattern: biofilm nutritional quality decreased significantly with increasing DOC, as indicated particularly by a decrease of the </span><span><em><span><span>w</span></span></em>-3:</span><span><em><span><span>w</span></span></em>-6 ratio and increase in LSAFA content. Algal biomass, in contrast, was mainly controlled by dissolved inorganic nitrogen (DIN) concentration, while DOC concentration was of minor importance. The ongoing browning process is inducing a dramatic reduction in the nutritional quality of the stream biofilm. Such degradation of the major high-quality food source available for stream consumers may reduce the trophic transfer efficiency in stream ecosystems, potentially extending across the stream-forest ecotone. </span></p>
On following pages: 74. Colombian Speckled Tree-rat (Pattonomys semivillosus); 75. Carriker's Speckled Tree-rat (Pattonomys carrikeri); 76. Yellow Speckled Tree-rat (Pattonomys flavidus); 77. Orinocan Speckled Tree-rat (Pattonomys punctatus); 78. Bare-tailed Tree-rat (Pattonomys occasius); 79. Peruvian Toro (Toromys rhipidurus); 80. Black Toro (Toromys grandis); 81. Dark Tree-rat (Echimys saturnus); 82. White-faced Tree-rat Echimys chrysurus), 83. Vieira's Tree-rat (Echimys vieirai): 84. Long-tailed Armored Tree-rat (Makalata macrura); 85. Red-nosed Armored Tree-rat (Makalata didelphoides); 86. Dark Armored Tree-rat (Makalata obscura). in Echimyidae
On following pages: 74. Colombian Speckled Tree-rat (Pattonomys semivillosus); 75. Carriker's Speckled Tree-rat (Pattonomys carrikeri); 76. Yellow Speckled Tree-rat (Pattonomys flavidus); 77. Orinocan Speckled Tree-rat (Pattonomys punctatus); 78. Bare-tailed Tree-rat (Pattonomys occasius); 79. Peruvian Toro (Toromys rhipidurus); 80. Black Toro (Toromys grandis); 81. Dark Tree-rat (Echimys saturnus); 82. White-faced Tree-rat Echimys chrysurus), 83. Vieira's Tree-rat (Echimys vieirai): 84. Long-tailed Armored Tree-rat (Makalata macrura); 85. Red-nosed Armored Tree-rat (Makalata didelphoides); 86. Dark Armored Tree-rat (Makalata obscura).
FIGURE. Morphology of Marchantia species of Sri Lanka. (A) Yellowish green, robust thallus of M. acaulis with a distinct dark median band and dark purplish margin (B) Light green thallus of M. paleacea without a distinct median band (C) Thallus of M. papillata with a distinct black coloured median band (D) Pale green coloured thallus of M. pappeana without a distinct median band (E) Dark green thallus of M. polymorpha (F) Green coloured thallus of M. emarginata with a blackish median band. A—Ruklani & Rubasinghe 108-14SR; B—Ruklani & Rubasinghe 14-14SR; C—Ruklani & Rubasinghe 28-14SR; D—Ruklani & Rubasinghe 55-14SR; E—Ruklani & Rubasinghe 360-15SR; F—Ruklani & Rubasinghe 169-14SR. in Thalloid Liverworts (Marchantiopsida) of Sri Lanka
FIGURE. Morphology of Marchantia species of Sri Lanka. (A) Yellowish green, robust thallus of M. acaulis with a distinct dark median band and dark purplish margin (B) Light green thallus of M. paleacea without a distinct median band (C) Thallus of M. papillata with a distinct black coloured median band (D) Pale green coloured thallus of M. pappeana without a distinct median band (E) Dark green thallus of M. polymorpha (F) Green coloured thallus of M. emarginata with a blackish median band. A—Ruklani & Rubasinghe 108-14SR; B—Ruklani & Rubasinghe 14-14SR; C—Ruklani & Rubasinghe 28-14SR; D—Ruklani & Rubasinghe 55-14SR; E—Ruklani & Rubasinghe 360-15SR; F—Ruklani & Rubasinghe 169-14SR.
FIGURE. Dumortiera hirsuta (Sw.) Nees II. Dark green, dichotomously branched thalli with a greasy appearance Ruklani & Rubasinghe 84-14R (PDA) in Thalloid Liverworts (Marchantiopsida) of Sri Lanka
FIGURE. Dumortiera hirsuta (Sw.) Nees II. Dark green, dichotomously branched thalli with a greasy appearance Ruklani & Rubasinghe 84-14R (PDA)
Distribution. Obi, Bisa, and Obilatu (= Obi-Latoe) Is in the NC Moluccas, Indonesia. Descriptiveor notes. Head-body 36-39 cm, tail 30-33.5 cm; weight 1.1-1.4 kg. The Obi Cuscus is a relatively small cuscus (condylobasal length 65-69 mm). Skull of the Obi Cuscus is similar to that of the Moluccan Cuscus (P. ornatus) and the Gebe Cuscus (P. alexandrae), and it bears a prominent diastema between incisor and canine but is smaller than those species and has smaller teeth. The Obi Cuscus has two color morphs: orange-brown or gray dorsal fur with dark underfur. Ventral fur is white to yellow. Dark dorsal stripe extends from head to mid-back or rump. in Phalangeridae
Distribution. Obi, Bisa, and Obilatu (= Obi-Latoe) Is in the NC Moluccas, Indonesia. Descriptiveor notes. Head-body 36-39 cm, tail 30-33.5 cm; weight 1.1-1.4 kg. The Obi Cuscus is a relatively small cuscus (condylobasal length 65-69 mm). Skull of the Obi Cuscus is similar to that of the Moluccan Cuscus (P. ornatus) and the Gebe Cuscus (P. alexandrae), and it bears a prominent diastema between incisor and canine but is smaller than those species and has smaller teeth. The Obi Cuscus has two color morphs: orange-brown or gray dorsal fur with dark underfur. Ventral fur is white to yellow. Dark dorsal stripe extends from head to mid-back or rump.
ScienceDex guides
Understand access before you commit
These curated guides explain access requirements, typical timelines, costs, and reuse considerations for widely used research datasets.
Allen Brain Atlas
Allen Brain Atlas is an Allen Institute collection of brain map atlases, datasets, APIs, and analysis tools covering mouse, human, and non-human primate brain resources.
Annotated Behaviour and Observability Dataset (ABODe)
ABODe is a University of Edinburgh DataShare dataset for behavior classification in group-housed mice using home-cage video, identities, bounding boxes, ground-plate positions, and annotator labels.
DANDI Archive for NWB datasets
DANDI is a BRAIN Initiative archive for publishing and sharing neurophysiology data, including electrophysiology, optophysiology, and behavioral data packaged as NWB and related standards.
International Brain Laboratory public data
The International Brain Laboratory public data releases expose standardized mouse decision-making experiments, including Neuropixels recordings, widefield calcium imaging, behavior, and session metadata accessed through the ONE API.
OpenNeuro
OpenNeuro is a free, open platform for sharing neuroimaging datasets, with public search, dataset pages, and download paths for web, S3, DataLad, and the OpenNeuro CLI.