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FIG. 7 in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 7. — Bayesian cladogram based on enteropneust 18S and 16S rRNA sequences, rooted using an echinoid echinoderm (Echinocrepis rostrata Mironov, 1973). Numbers at nodes represent posterior probabilities (p). All nodes with p<0.95 were collapsed into polytomies.
FIG. 3. — Tergivelum baldwinae n. gen., n in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 3. — Tergivelum baldwinae n. gen., n. sp. in approximate dorsal view: A, surface details; B, locations of major nerves and muscles associated with proboscis and collar. Abbreviations for structural features: see text.
FIG. 8 in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 8. — Single frame (at 5 min: 37 sec) of 8-min videotape of Tergivelum baldwinae n. gen., n. sp. paratype IV. Filled circles show path of a particle transported unobstructed about 5 cm above the bottom (from 5:47 to 5:53). Open circles show path of particle (small polychaete) drifting about 2 cm above the bottom and evidently getting stuck (at 5:36) in substantial mucus surrounding acorn worm;arrow indicates shadow cast on sea floor by the immobilized particle. Scale bar: 5 cm.
FIG. 6 in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 6. — Cross sections (B-J) of Tergivelum baldwinae n. gen., n. sp. at levels indicated in 4B: A, parasagittal section in region of gill pores showing primary gill bar with skeleton (arrowed) and secondary gill bar with skeleton (arrowheads) and coelomic space (asterisk); B, cross section of trunk near anterior extremity of ventral nerve cord (in rectangle); C, detail from rectangle in 6B with ventral nerve cord underlain by ventral blood vessel (arrowhead); D, cross section of anterior trunk showing dorsal protuberances and back veils (the left one broken off); dark spheres are testes; E-J, intestinal region of trunk; asterisks mark lateroventral folds); dorsal and ventral nerve cords indicated, respectively, by arrows and arrowheads; K, section through three testes; L, detail of testis with spermatozoafilled lumen toward top right; M, medium-sized oocytes; N, large oocyte. Abbreviations for structural features: see text. Scale bars: A, 100 μm; B, D, 1 mm; C, 50 μm; E-J, N, 500 μm; K, M, 200 μm; L, 20 μm.
FIG. 5 in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 5. — Cross sections of Tergivelum baldwinae n. gen., n. sp. at levels indicated in Figure 4B: A, near anterior tip of proboscis, arrow indicates tract of longitudinal muscle fibers; B, enlargement of rectangle in 5A showing epidermis (toward right) underlain by basal concentration (arrowed) of diffuse intraepidermal nervous system; proboscis coelom contains meshwork of connective tissue and muscle cells; C, more posterior section of proboscis; D, section through collar showing anterior end of right buccal muscle; specimen oriented with left side somewhat in advance of right, so left buccal muscle not yet in view; E, detail of the center rectangle in 5D; showing lumen of collar cord separating dorsal non-neural and ventral neural regions; perihaemal coeloms (marked by asterisks) lie on either side of dorsal blood vessel; F, detail of left-hand rectangle in 5D. Collar-trunk septum separates trunk coelom (above) from collar coelom (below); G, section through level of the mouth; lateral lips comprise ventral region of collar; posteroventral extremity of proboscis forms anterior margin of mouth; H, detail in the rectangle in 5G; beneath dorsal nerve cord is dorsal blood vessel with parts of trunk coelom (asterisks) on either side; I, section at level of posterior rim of mouth; buccal muscles approaching each other and will merge a few sections more posteriorly; pharynx comprising ventral digestive region (arrowheads) and dorsal branchial region (obliquely sectioned) penetrated by gill pores. Abbreviations for structural features: see text. Scale bars: A, C, D, G, I, 1 mm; B, 50 μm; E, 100 μm; F, 300 μm; H, 200 μm.
FIG. 4 in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 4. — Fixed specimens of Tergivelum baldwinae n. gen., n. sp.: A, holotype (ventral view) which broke into three parts when fixed – namely the left back veil (lbv), most of intestinal region of trunk (at right), and anterior body (at left, comprising proboscis, collar, and anterior extremity of trunk); B, holotype (dorsal view, excluding left back veil) with numbered letters indicating levels of cross section in Figures 5 and 6; C, enlargement of anterior portion of holotype in ventral view; lateral lips of collar (arrowheads) curl dorsally as a preservation artifact; D, enlargement of anterior portion of the holotype in dorsal view; arrows indicate dorsal protuberances; E, enlargement of anterior portion of holotype in left side view with arrow indicating fossa of left proboscis nerve; F, dorsal view of anterior region of trunk of paratype II (corresponding to area in rectangle in panel 4D); back veils and dorsal protuberances dissected away revealing dorsal nerve cord (arrowed) flanked by slot-shaped gill pores. Abbreviations for structural features: see text. Scale bars: A, B, 1 cm; C-F, 2 mm.
FIG. 2 in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 2. — Single video frames of living Tergivelum baldwinae n. gen., n. sp.: A, anterior of paratype IV, white arrowhead indicates fossa of left proboscis nerve; B, holotype laying down fecal trail; suction sampler in background; C, paratype II laying down fecal trail, 29 cm between red laser dots. Abbreviations: co, collar; lbv, left back veil; pr, proboscis; rlf, right lateroventral fold. Scale bars: A, 2 cm; B, C, 3 cm.
FIG. 1 in A new deep-sea species of epibenthic acorn worm (Hemichordata, Enteropneusta)
FIG. 1. — Collection site (depth: 3952-3953 m) for holotype and paratypes I-VI of Tergivelum baldwinae n. gen., n. sp.
Figure 9 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 9. Development of the endogenous ovary in Epiperipatus biolleyi. Transmission electron micrographs. A, position of the ovarian anlage beneath the presumptive heart and attached to the pericardial floor (pe) in an embryo with a full number of somites. Cross-section of the dorsal body. B, cross-section of an ovarian tube. Note the distinct separation into a germinal epithelium (ge), which contains the primordial germ cells (pgc), and a sterile epithelium (se). C, detail of the sterile epithelium. D, detail of the germinal epithelium. Arrowheads indicate apical junctions. Abbreviations: bl, basal lamina; ec, ectoderm; ge, germinal ovarian epithelium; hc, haemocoel; hl, lumen of the presumptive heart; lu, lumen of the ovarian anlage; me, outer layer of mesodermal cells that will later form the ovarian musculature; nu, nucleus; pe, presumptive pericardial floor; pgc, primordial germ cells; se, sterile ovarian epithelium.
Figure 7 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 7. Internal organization of the endogenous ovary in Epiperipatus biolleyi. Light micrograph (A) and transmission electron micrographs (B–F). A, cross-section of the ovary (dorsal is up). Note the central position of ovarian lumen (lu) surrounded by germinal epithelium (ge) and the lack of a sterile epithelium. B, maturating oocyte (oc) from the germinal epithelium lying within a spherical chamber (ch), which is formed by specific cells (ce) of the germinal epithelium. C, detail of epithelial cells and an oocyte. Arrowheads indicate apical junctions. D, detail of the basal portion of the germinal epithelium with surrounding connective tissue containing muscle cells (mc). E, lower magnification of connective tissue showing numerous tracheal tubes (arrows). F, peripheral region of connective tissue containing tracheal tubes (tr) and flattened cells with an electron-dense content (fc). Abbreviations: bl, basal lamina; ce, cells of germinal epithelium that form the oocyte chamber; ch, oocyte chamber; ct, connective tissue; fc, flattened cell; ge, germinal epithelium; hc, haemocoel; lu, ovarian lumen; mc, muscle cells; mv, microvilli; nl, nucleolus; nu, nucleus; oc, maturating oocytes; tr, tracheal tubes.
Figure 5 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 5. Internal organization of the exogenous ovary in Opisthopatus roseus (A–C, E, F) and Peripatopsis balfouri (D). Transmission electron micrographs. A, detail of ovarian epithelia and lumen. Arrowheads indicate apical junctions connecting epithelial cells. B, mitotically dividing oogonium (og) from the germinal epithelium. C, maturating oocyte (oc) with associated cells (ce) of modified germinal epithelium. Arrows point to the basal lamina which is strongly folded. D, maturating oc in the process of breaking through the connective tissue and growing out into the haemocoel. E, detail of dorsal ovarian wall showing the sterile epithelium (se) and the connective tissue (ct), which contains the musculature (mc). F, higher magnification of connective tissue showing muscle cells and collagen fibres. Abbreviations: bl, basal lamina; ce, cells associated with an oocyte (sometimes referred to as 'follicle cells' in the literature); cg, collagen fibres; ct, connective tissue; ge, germinal epithelium; hc, haemocoel; he, haemocyte; lu, ovarian lumen; mc, muscle cell; mt, mitochondria; mv, microvilli; nl, nucleolus; nu, nucleus; oc, maturating oocyte; og, oogonium; se, sterile epithelium; st, growing stalk.
Figure 4 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 4. Internal organization of the exogenous ovary in Opisthopatus roseus (A, B) and Peripatopsis balfouri (C). Transmission electron micrographs. A, cross-section through the middle of the ovary. Dorsal is up. Note the unpaired lumen (lu) and the separation of the ovarian epithelium into a dorsal sterile epithelium (se) and a ventral germinal epithelium (ge). B, stalked oocytes enclosed by a vitelline membrane (= primary egg membrane). C, detail of a stalk. Arrows indicate intermediate filaments, arrowheads point to hemidesmosomes. Inset shows continuity of the basal lamina covering a stalk and a maturating oocyte that bulges into the haemocoel of the female. Abbreviations: bl, basal lamina; ct, connective tissue; ge, germinal epithelium; hc, haemocoel; lu, ovarian lumen; nl, nucleolus; nu, nucleus; oc, maturating oocytes; se, sterile epithelium; st, stalk; vm, vitelline membrane.
Figure 6 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 6. Internal organization of the pseudoendogenous ovary in Metaperipatus inae (A–E) and Metaperipatus blainvillei (F). Light micrographs (A, B) and transmission electron micrographs (C–F). A, cross-section of the ovary (dorsal is up). Note the lateral position of the crescent-shaped ovarian lumen (lu) and the central position of the germinal epithelium (ge). B, detail of stalked oocytes (oc) from the germinal epithelium, which do not bulge into the haemocoel but retain their position within the ovary. C, detail of cells (ce) surrounding a maturating oocytes in the germinal epithelium. D, detail of a stalk. Arrows indicate the intermediate filaments. E, detail of the lumen and ovarian epithelia. The epithelial cells are connected by an apical junction (arrowhead). F, lateral ovarian wall consisting of the sterile epithelium (se) and connective tissue containing muscle cells (mc), a haemocyte (he), and sperm (sh). Abbreviations: bl, basal lamina; ce, cells associated with an oocyte; cg, collagen fibres; ct, connective tissue; ge, germinal epithelium; hc, haemocoel; he, haemocyte; lu, ovarian lumen; mc, muscle cell; mv, microvilli; nl, nucleolus; nu, nucleus; oc, maturating oocyte; se, sterile epithelium; sh, sperm head; st, stalk; sw, sterile ovarian wall.
Figure 3 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 3. Diagram of internal organization of the three major ovarian types in Onychophora: exogenous ovary (A, D), pseudoendogenous ovary (B, E), and endogenous ovary (C, F). A, cross-section of the exogenous ovary with separate ovarian tubes that occur, e.g. in Euperipatoides rowelli, Phallocephale tallagandensis, and Ooperipatellus insignis (Australian Peripatopsidae). B, cross-section of the pseudoendogenous ovary of Metaperipatus inae (Peripatopsidae, Chile). C, cross-section of the endogenous ovary of Epiperipatus biolleyi (Peripatidae, Costa Rica). Note the complete lack of a sterile epithelium. D, detail of the composition of the ovarian wall in Opisthopatus roseus (Peripatopsidae, South Africa). E, detail of the ovary in Met. inae. F, detail of the ovarian wall in Ep. biolleyi. Abbreviations: bl, basal lamina; ct, connective tissue; fc, flattened cell; ge, germinal epithelium; hc, haemocoel; lu, ovarian lumen; mc, muscle cell; oc, oocyte; se, sterile epithelium; st, stalk; tr, tracheae.
Figure 1 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 1. Simplified diagrams of paired versus variously fused structure of the ovarian tubes in Onychophora. Tissues are represented in light grey, ovarian lumen in dark grey. A, exogenous ovary of Typhloperipatus williamsoni (South-East Asian Peripatidae). Modified and complemented according to descriptions given by Kemp (1914). B–D, exogenous ovaries in three species of Peripatopsidae. B, Euperipatoides rowelli (Australia). Note the completely separate ovarian tubes in the middle of the ovary and the fused ovarian lumens at the anterior and posterior ends. A similar ovarian organization has been described in Peripatoides novaezealandiae from New Zealand (Sheldon, 1890: fig. 26). C, Peripatopsis balfouri (South Africa, cf. Fig. 2A). Although the ovarian tubes are fused, their lumens are separate along their entire length. D, Opisthopatus roseus (South Africa). Note the unpaired ovarian structure with a single lumen. E, pseudoendogenous ovary of Metaperipatus inae (Peripatopsidae, Chile, cf. Fig. 2B) with fused ovarian tubes but separate lumens. F, endogenous ovary of Epiperipatus biolleyi (Neotropical Peripatidae, cf. Fig. 2C) with lumens communicating only at the posterior end. G, endogenous ovary of Mesoperipatus tholloni (Peripatidae, Tropical Africa), modified and complemented after Bouvier (1905). Each ovarian tube is completely separate in this species.
Figure 10 in Position and development of oocytes in velvet worms shed light on the evolution of the ovary in Onychophora and Arthropoda
Figure 10. Mapping of three major types of onychophoran ovaries on simplified trees representing three different hypotheses on the phylogenetic relationships of Onychophora. Onychophoran subgroups are designated by their geographical distribution. Note that the suggestion of the exogenous type as an ancestral feature of Onychophora is consistent with all three phylogenetic hypotheses. A, both Peripatopsidae and Peripatidae are monophyletic (phylogeny modified from Monge-Nájera, 1995: fig. 10). B, Peripatidae are nonmonophyletic (phylogeny simplified from Reid, 1996: fig. 29). C, Peripatopsidae are nonmonophyletic (phylogeny simplified from Reid, 1996: fig. 28).
Liver fluke (Opisthorchis viverrini) worm burdens and egg counts from humans in Thailand and Lao PDR
<p>Helminth transmission and morbidity are dependent on the number of mature parasites within a host, however, observing adult worms is impossible for many natural infections. An outstanding challenge is therefore relating routine diagnostics, such as faecal egg counts, to the underlying worm burden. This relationship is complicated by density-dependent fecundity (egg output per-worm reduces due to crowding at high burdens) and the skewed distribution of parasites (majority of helminths aggregated in a small fraction of hosts). We address these questions for the carcinogenic liver fluke <em>Opisthorchis viverrini</em>, which infects approximately ten million people across Southeast Asia, by analysing five epidemiological surveys (<em>n </em>= 641) where adult flukes were recovered. Using a mechanistic model, we show that parasite fecundity varies between populations, with surveys from Thailand and Laos demonstrating distinct patterns of egg output and density-dependence. As the probability of observing faecal eggs increases with the number of mature parasites within a host, we quantify diagnostic sensitivity as a function of the worm burden and find that > 50% of cases are misdiagnosed as false negative in communities close to elimination. Finally, we demonstrate that the relationship between observed prevalence from routine diagnostics and true prevalence is non–linear and strongly influenced by parasite aggregation.</p>
Figure 4 in Mezcal worm in a bottle: DNA evidence suggests a single moth species
Figure 4 Lateral view of a Comadia redtenbacheri larva showing three key features useful to distinguish it from other mezcal worms. Photo by Jose I. Martinez.
Figure 5 in Mezcal worm in a bottle: DNA evidence suggests a single moth species
Figure 5 Maximum likelihood tree showing the placement of the 18 successfully sequenced mezcal worms (in bold and red) in relationship to publicly available COI sequences of Comadia redtenbacheri (Hammerschmidt) and related Cossidae species. Scale bar = number of substitutions/site. Photo by Jose I. Martinez.
Figure 1 in Mezcal worm in a bottle: DNA evidence suggests a single moth species
Figure 1 Adults of three insects species presumed to be the mezcal worm. (A) Comadia redtenbacheri (Cossidae), (B) Aegiale hesperiaris (Hesperiidae), (C) Scyphophorus acupunctatus (Curculionidae). Photo credits (from (A C), respectively): Mark Rosenstein, Big Bend, Brewster, Texas, USA; Ricardo Arredondo T., Coeneo, Michoacan, México; Simon Oliver, Yegen, Granada, Spain.
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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.