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543 results for “larval development”
Effects of embryo energy, egg size and larval food supply on the development of asteroid echinoderms
Organisms have limited resources available to invest in reproduction, causing a tradeoff between the number and size of offspring. One consequence of this tradeoff is the evolution of disparate egg sizes and, by extension, developmental modes. In particular, echinoid echinoderms (sea urchins and sand dollars) have been widely used to experimentally manipulate how changes in egg size affect development. Here we test the generality of the echinoid results by 1) using laser ablations of blastomeres to experimentally reduce embryo energy in the asteroid echinoderms (sea stars), Pisaster ochraceus and Asterias forbesi and 2) comparing naturally produced, variably-sized eggs (1.7 fold volume difference between large and small eggs) in A. forbesi. In P. ochraceus and A. forbesi there were no significant differences between juveniles from both experimentally reduced embryos and naturally produced eggs of variable size. However, in both embryo reduction and egg size variation experiments, simultaneous reductions in larval food had a significant and large effect on larval and juvenile development. These results indicate that 1) food levels are more important than embryo energy or egg size in determining larval and juvenile quality in sea stars and 2) the relative importance of embryo energy or egg size to fundamental life history parameters (time-to and size-at metamorphosis), does not appear to be consistent within echinoderms.
Severe hypoxia exposure inhibits larval brain development but does not affect the capacity to mount a cortisol stress response in zebrafish
<p>Fish nursery habitats are increasingly hypoxic and the brain is recognized as highly hypoxia-sensitive, yet there is a lack of information on the effects of hypoxia on the development and function of the larval fish brain. Here, we tested the hypothesis that by inhibiting brain development, larval exposure to severe hypoxia has persistent functional effects on the cortisol stress response in zebrafish (<i>Danio rerio</i>). Exposing 5 days post-fertilization (dpf) larvae to 10% dissolved O<sub>2</sub> (DO) for 16 h only marginally reduced survival, but it decreased forebrain neural proliferation by 55%, and reduced the expression of <i>neurod1</i>, <i>gfap,</i> and <i>mbpa, </i>markers of determined neurons, glia, and oligodendrocytes, respectively. The 5 dpf hypoxic exposure also elicited transient increases in whole body cortisol and in <i>crf</i>, <i>uts1</i>, and <i>hsd20b2</i> expression, key regulators of the endocrine stress response. Hypoxia exposure at 5 dpf also inhibited the cortisol stress response to hypoxia in 10 dpf larvae and increased hypoxia tolerance. However, 10% DO exposure at 5 dpf for 16h did not affect the cortisol stress response to a novel stressor in 10 dpf larvae or the cortisol stress response to hypoxia in adult fish. Therefore, while larval exposure to severe hypoxia can inhibit brain development, it also increases hypoxia tolerance. These effects may transiently reduce the impact of hypoxia on the cortisol stress response but not its functional capacity to respond to novel stressors. We conclude that the larval cortisol stress response in zebrafish has a high capacity to cope with severe hypoxia-induced neurogenic impairment.</p>
FIGURE 7 in Description of the complete larval development of Lysmata amboinensis (De Man) (Decapoda: Lysmatidae) reared under laboratory conditions
FIGURE 7. Decapodite: A specimen lateral view; A' complete specimen lateral view; B antennule; C antenna; D mandibles; E maxillule; F maxilla; G first maxilliped; H second maxilliped; I third maxilliped; J first pereiopod; J' first pereiopod, detail of chelae; K second pereiopod; K' second pereiopod, detail of chelae; L third pereiopod; L' third pereiopod, detail of chelae; M fourth pereiopod; M' fourth pereiopod, detail of chelae; N fifth pereiopod; N' fifth pereiopod, detail of chelae; O first pleopod; P second pleopod; Q third pleopod; R fourth pleopod; S fifth pleopod; T telson; U uropods. Scale bars: 0.1mm.
FIGURE 6 in Description of the complete larval development of Lysmata amboinensis (De Man) (Decapoda: Lysmatidae) reared under laboratory conditions
FIGURE 6. Tenth zoea: A complete larvae lateral view; B rostrum and carapace denticles; C antennule; D antenna; E mandibles; F maxillule; G maxilla; H first maxilliped; I second maxilliped; J third maxilliped; K first pereiopod; L second pereiopod; M third pereiopod; N fourth pereiopod; O fifth pereiopod; P first pleopod; Q second pleopod; R third pleopod; S fourth pleopod; T fifth pleopod; U telson and uropods. Scale bars: 0.1mm.
FIGURE 4 in Description of the complete larval development of Lysmata amboinensis (De Man) (Decapoda: Lysmatidae) reared under laboratory conditions
FIGURE 4. Sixth zoea: A antennule; B mandibles; C third pereiopod; D fourth pereiopod; E uropods and telson. Seventh zoea: F larvae dorsal view; G maxillule; H maxilla. Scale bars: 0.1mm.
FIGURE 2 in Description of the complete larval development of Lysmata amboinensis (De Man) (Decapoda: Lysmatidae) reared under laboratory conditions
FIGURE 2. Second zoea: A complete larvae dorsal view; B antenna; C mandibles; D pleon lateral view; E first pereiopod; F fifth pereiopod. Third zoea: G antennule; H mandibles; I maxilla; J first pereiopod; K fifth pereiopod; L telson and uropods. Scale bars: 0.1mm.
FIGURE 1 in Description of the complete larval development of Lysmata amboinensis (De Man) (Decapoda: Lysmatidae) reared under laboratory conditions
FIGURE 1. First zoea: A complete larvae lateral view; A' carapace denticles; B antennule; C antenna; D mandibles; E maxillule; F maxilla; G first maxilliped; H second maxilliped; I third maxilliped; J telson. Scale bars: 0.1mm (A–D, F–J); 0.5mm (E).
FIGURE 5 in Description of the complete larval development of Lysmata amboinensis (De Man) (Decapoda: Lysmatidae) reared under laboratory conditions
FIGURE 5. Eighth zoea: A antennule; B antenna; C mandibles. Ninth zoea: D larvae dorsal view; E first maxilliped; F pleopods. Scale bars: 0.1mm.
FIGURE 3 in Description of the complete larval development of Lysmata amboinensis (De Man) (Decapoda: Lysmatidae) reared under laboratory conditions
FIGURE 3. Fourth zoea: A complete larvae lateral view; B antenna; C mandibles; D detail of fifth's pereiopod propodus and dactylus. Fifth zoea: E antennule; F first maxilliped; G second pereiopod; H third pereiopod; I detail of fifth's pereiopod propodus and dactylus; J uropods and telson. Scale bars: 0.1mm.
Data from: Correlated evolution of larval development, egg size, and genome size across two genera of snapping shrimp
<p>Across plants and animals, genome size is often correlated with life history traits: large genomes are correlated with larger seeds, slower development, larger body size, and slower cell division. Among decapod crustaceans, caridean shrimps are among the most variable both in terms of genome size variation and life history characteristics such as larval development mode and egg size, but the extent to which these traits are associated in a phylogenetic context is largely unknown. In this study, we examine correlations among egg size, larval development, and genome size in two different genera of snapping shrimp, <em>Alpheus </em>and <em>Synalpheus, </em>using phylogenetically informed analyses<em>. </em>In both <em>Alpheus </em>and <em>Synalpheus, </em>egg size is strongly linked to larval development mode: species with abbreviated development had significantly larger eggs than species with extended larval development. We produced the first comprehensive dataset of genome size in <em>Alpheus </em>(n = 37 species), and demonstrated that genome size was strongly and positively correlated with egg size in both <em>Alpheus </em>and <em>Synalpheus. </em>Correlated trait evolution analyses showed that in <em>Alpheus</em>, changes in genome size were clearly dependent on egg size. In <em>Synalpheus, </em>evolutionary path analyses suggest that changes in development mode (from extended to abbreviated) drove increases in egg volume; and larger eggs, in turn, resulted in larger genomes. These data suggest that variation in reproductive traits may underpin the high degree of variation in genome size seen in a wide variety of caridean shrimp groups more generally.</p>
FIGURE 7 in Larval development of the crab Amphithrax hemphilli (Rathbun, 1892) (Decapoda, Brachyura, Mithracidae) described from laboratory-reared material
FIGURE 7. Cladogram of species of Mithrax and allies for the megalopa stage, with phylogeny constructed from Windsor & Felder (2014) and Assugeni et al. (2017). Characteristics: (1) setae on the peduncle of the antennule; (2) aesthetascs on the exopod of the antennule; (3) setation of the antenna; (4) setae on the palp of the mandible; (5) setae on the coxal endite of the maxillule; (6) setae on the basial endite of the maxillule; (7) setae on the endopod of the maxillule; (8) setae on the epidod of the maxillule; (9) setae on the coxal endite of the maxilla; (10) setae on the basial endite of the maxilla; (11) setae on the endopod of the maxilla; (12) setae on the scaphognathite of the maxilla; (13) setae on the basis of the first maxilliped; (14) setae on the endopod of the first maxilliped; (15) setae on the exopod of the first maxilliped; (16) setae on the endopod of the second maxilliped; (17) setae on the exopod of the second maxilliped; (18) setae on the coxa of the third maxilliped; (19) setae on the basischium of the third maxilliped; (20) setae on the endopod of the third maxilliped; (21) setae on the exopod of the third maxilliped, and (22) setae on the pleon. Different colors indicate differences among species; equal colors indicate similarity.
FIGURE 4 in Larval development of the crab Amphithrax hemphilli (Rathbun, 1892) (Decapoda, Brachyura, Mithracidae) described from laboratory-reared material
FIGURE 4. Amphithrax hemphilli (Rathbun, 1892), megalopa stage. (A) maxilliped I; (B) maxilliped II; (C) maxilliped III; (D) pleopods 1–4 and uropod; (E) pereiopods 1–5; (F) dorsal and lateral view of pleon and telson. Scale bars: A–C: 0.1 mm; D–F: 0.2 mm.
FIGURE 1 in Larval development of the crab Amphithrax hemphilli (Rathbun, 1892) (Decapoda, Brachyura, Mithracidae) described from laboratory-reared material
FIGURE 1. Amphithrax hemphilli (Rathbun, 1892), first zoeal stage. (A) Lateral view; (B) dorsal view; (C) antennule; (D) antenna; (E) mandible; (F) maxillule (G) maxilla; (H) maxilliped I; (I) maxilliped II; (J) maxilliped III; (K) pereiopods; (L) dorsal view of pleon and telson. Scale bars: A, B, L: 0.2 mm; C–K: 0.1 mm.
FIGURE 6 in Larval development of the crab Amphithrax hemphilli (Rathbun, 1892) (Decapoda, Brachyura, Mithracidae) described from laboratory-reared material
FIGURE 6. Cladogram of species of Mithrax and allies for the second zoeal stage, with phylogeny constructed from Windsor & Felder (2014) and Assugeni et al. (2017). Characteristics: (1) setae on the anterodorsal region of the carapace; (2) setae on the posterodorsal region of the carapace; (3) setae on the ventral margin of the carapace; (4) aesthetascs on the antennule; (5) setae on the antennule; (6) setae on the coxal endite of the maxillule; (7) setae on the basial endite of the maxillule; (8) setae on the endopod of the maxillule; (9) setae on the coxal endite of the maxilla; (10) setae on the basial endite of the maxilla; (11) setae on the endopod of the maxilla; (12) setae on the scaphognathite of the maxilla; (13) setae on the coxa of the first maxilliped; (14) setae on the basis of the first maxilliped; (15) setae on the endopod of the first maxilliped; (16) setae on the coxa of the second maxilliped; (17) setae on the basis of the second maxilliped, and (18) setae on the endopod of the second maxilliped. Different colors indicate differences among species; equal colors indicate similarity.
FIGURE 2 in Larval development of the crab Amphithrax hemphilli (Rathbun, 1892) (Decapoda, Brachyura, Mithracidae) described from laboratory-reared material
FIGURE 2. Amphithrax hemphilli (Rathbun, 1892), second zoeal stage. (A) Lateral view; (B) antennule; (C) antenna; (D) mandible; (E) maxillule (F) maxilla; (G) maxilliped I; (H) maxilliped II; (I) maxilliped III; (J) pereiopods; (K) dorsal view of pleon and telson. Scale bars: A, J, K: 0.2 mm; B–I: 0.1 mm.
FIGURE 5 in Larval development of the crab Amphithrax hemphilli (Rathbun, 1892) (Decapoda, Brachyura, Mithracidae) described from laboratory-reared material
FIGURE 5. Cladogram of species of Mithrax and allies for the first zoeal stage, with phylogeny constructed from Windsor & Felder (2014) and Assugeni et al. (2017). Characteristics: (1) setae on the anterodorsal region of the carapace; (2) setae on the posterodorsal region of the carapace; (3) setae on the ventral margin of the carapace; (4) aesthetascs on the antennule; (5) setae on the antennule; (6) setae on the coxal endite of the maxillule; (7) setae on the basial endite of the maxillule; (8) setae on the endopod of the maxillule; (9) setae on the coxal endite of the maxilla; (10) setae on the basial endite of the maxilla; (11) setae on the endopod of the maxilla; (12) setae on the scaphognathite of the maxilla; (13) setae on the coxa of the first maxilliped; (14) setae on the basis of the first maxilliped; (15) setae on the endopod of the first maxilliped; (16) setae on the coxa of the second maxilliped; (17) setae on the basis of the second maxilliped, and (18) setae on the endopod of the second maxilliped. Different colors indicate differences among species; equal colors indicate similarity.
FIGURE 7. Petrolisthes tuberculatus. Pereiopods, zoea II, A in Larval development of Petrolisthes tuberculatus (Guérin, 1835) (Decapoda, Anomura, Porcellanidae) reared in laboratory
FIGURE 7. Petrolisthes tuberculatus. Pereiopods, zoea II, A; Pereiopods, megalopa, B. Fifth pereiopod dactylus detail, megalopa, C. Sternum, megalopa, D. Pleon, pleopods and telson, zoea I, E; Pleon, pleopods and telson, zoea II, F.1, F.2; Pleon, pleopods and telson, megalopa, G. Scale bars: A, G = 0.5 mm.; B, D, E, F.1 = 1 mm; C, F.2 = 0.2 mm.
FIGURE 5. Petrolisthes tuberculatus. Maxilla, zoea I, A in Larval development of Petrolisthes tuberculatus (Guérin, 1835) (Decapoda, Anomura, Porcellanidae) reared in laboratory
FIGURE 5. Petrolisthes tuberculatus. Maxilla, zoea I, A; Maxilla, zoea II, B; Maxilla, megalopa, C. First maxilliped, zoea I, D; First maxilliped, zoea II, E; First maxilliped, megalopa, F. Scale bars: A-C, F = 0.2 mm; D, E = 0.5 mm.
FIGURE 4. Petrolisthes tuberculatus. Mandibles, zoea I, A in Larval development of Petrolisthes tuberculatus (Guérin, 1835) (Decapoda, Anomura, Porcellanidae) reared in laboratory
FIGURE 4. Petrolisthes tuberculatus. Mandibles, zoea I, A; Mandibles, zoea II, B; Mandibles, megalopa, C. Maxillule, zoea I, D; Maxillule, zoea II, E; Maxillule, megalopa, F. Scale bars: 0.2 mm.
FIGURE 2 in Larval development of Petrolisthes tuberculatus (Guérin, 1835) (Decapoda, Anomura, Porcellanidae) reared in laboratory
FIGURE 2. Petrolisthes tuberculatus. General view: Zoea I, A; Zoea II, B; Megalopa, C, D. Rostrum of megalopa, E. Scale bars: 1 mm.
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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.
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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.
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