This work was funded in part by NIH R01 #DE021475 to CTM and an NSF Graduate Research Fellowship to NAE. Thanks to Miles Johnson for assistance with imaging and Priscilla Erickson for critical reading of the manuscript.

Todo o trabalho de peixe foi aprovado pelo Comitê Institucional de Animal Care and Use da Universidade da Califórnia-Berkeley (número de protocolo R330). A eutanásia foi realizada por meio de imersão em 0,025% tricaina-S tamponada com 0,1% de bicarbonato de sódio 39. Todos os passos são realizados à temperatura ambiente. 1. Preparação Nota: Execute as etapas 1,1-1,5 em tubos cônicos ou frascos de cintilação que pode selar firmemente e ser colocados na horizontal. Os peixes não precisam ser constantemente abalado, mas tente misturar a solução o mais rápido possível invertendo delicadamente ou sacudindo o rack de tubos ou frascos para expor todos os lados do peixe para a solução de coloração e permitir que mancha para penetrar no tecido uniformemente. Não coloque um grande lote de peixes em um agitador de plataforma, como o peso pesado do líquido vai quebrar o shaker. <ol><li> Fixar qualquer peixe recém-sacrificados ou peixe armazenado em etanol com 10% tamponada neutra de formalina (NBF) durante a noite. Como alternativa, use 4% paraformaldeído em solução 1x PBS em vez de NBF a 10%. Nota: Se extrair DNA, grampear uma pequena porção dos caudais ou barbatanas peitorais antes da fixação e armazenar em etanol. </li><li> Dispor de correção adequadamente em uma capa química e substituir com água da torneira (ou seja ~ pH 7,0) durante 2 horas. Evitar o uso de água deionizada, pois muitas vezes pode ser ácida e pode descalcificação óssea. </li><li> Retire a água e peixes mancha com 0,008% Alizarina S em 1% KOH em água por 24 horas. Para os peixes menos de 20 mm de comprimento padrão, utilize 0,004% Alizarina Red S. (Faça uma solução 100x (0,8%) de ações de Alizarina S, que pode então ser diluído). </li><li> Remova a mancha (colocar em um recipiente adequado de lixo na capa) e colocar peixes na água da torneira para alguns hr. Mudar a água como necessário até lavagem com água é mais clara. </li><li> Retire a água e coloque o peixe até 50% de glicerol, 0,25% KOH para limpeza suave e dissecção posterior. Nota: Este protocolo de coloração é modificado a partir de métodos anteriormente descritos 40,41. </li></ol><pclass = &quot;jove_title&quot;&gt; 2. dissecação Nota: Consulte a Figura 1 para uma revisão de cabeça relevante morfologia do esqueleto. <img alt="figura 1" src="/files/ftp_upload/54056/54056fig1.jpg" /> Figura 1:. Cabeça Stickleback morfologia do esqueleto Alizarina Red manchado cabeça Gasterosteus aculeatus fotografada com fluorescência sob um conjunto rodamina filtro B. morfologia útil é rotulado: Op = opérculo, Subop = subopercle, BSRs = branchiostegal raios, pré-operatório = preopérculo, Infraorb 1-3 = infraorbitários 1-3 (também chamados circumorbitals ou suborbitals), Dent = dentário, Premax = pré-maxila, Max = maxila , Nas = nasal, Lat. ethm = etmóide lateral, PSPH = paresfenóide, Fron = osso frontal. Para uma descrição mais detalhada da cabeça de esqueleto stickleback, consulte Anker (1974) 31. <a href="https://www.jove.com/files/ftp_upload/54056/54056fig1large.jpg" target="_blank">Por favor clique aqui para ver uma versão maior</a>esta figura. <ol><li> Deite o peixe plana (Figura 2A) e inserir uma pinça afiada # 5 de relojoeiro para o lado do olho com um ângulo de ~ 45 ° para perfurar a membrana que cobre o olho. </li><li> Descascar a membrana afastada, a partir do olho, semelhante à da casca de uma tampa de iogurte (Figura 2B). </li><li> Inserir uma pinça aberta atrás do olho, agarrar o nervo óptico por trás do olho, e remover o olho (Figura 2C). Não perfure o olho como ele vai vazar melanina. Se perfurado, a melanina pode ser lavado durante as etapas posteriores. </li><li> Repita do outro lado. </li><li> A partir do posterior, coloque uma lâmina de dissecação tesoura pequena sob a aba opérculo, lâmina de arrastar tesoura dorsal acima opérculo, em seguida, corte de tecidos moles até a órbita do olho (Figura 2D). Corte dorsal ao osso opérculo. </li><li> Cortar o osso frontal (dorsal para a cavidade ocular) (Figura 2E). </li><li> Cortar o osso paresfenóide linha média em torno de tEle centro das órbitas (Figura 2F). </li><li> corte opercle Repita no lado oposto. </li><li> Inserir uma pinça sob o opérculo e lentamente descascar o rosto para longe do corpo, aparando qualquer tecido mole ainda ligado (Figura 2G - H). Tome cuidado para não perturbar a primeira linha de rastros branquiais. <ol><li> Com uma pinça, retire as ceratohyals em ambos os lados do basihyal linha média, enquanto descascando e remover o esqueleto craniofacial anterior (toda a mandíbula, incluindo o dentário, pré-maxila, e da maxila; o esqueleto inteiro hióide incluindo o opérculo dérmica exterior, preopérculo, subopercle e raios branchiostegal e dorsal subjacente e elementos endocondrais ventral; e a parte anterior do crânio, incluindo o nasal, etmóide lateral e ossos infraorbital, ver figuras 1 e 2I). </li><li> espinhas pélvico pode ser dobrada para fora do corpo, e pode servir como um identificador para uma pinça para agarrar of quando presente. Espinhos encaixado. Para desbloquear, puxe coluna com uma pinça diretamente para fora do corpo do peixe, em seguida, dobre posteriormente para pressionar espinha plana contra peixes. </li></ol></li><li> Inserir fechada forceps posterior e ventral ao esqueleto branquial (logo abaixo tubo digestivo) e pinça de arrasto anteriormente, provocando além dos músculos restantes e ligamentos ligados ao esqueleto branquial (Figura 2J - K). </li><li> Usando as pontas de uma pinça fechadas, raspar os músculos que prendem a dorsal esqueleto branquial à caixa craniana ventral em um posterior à direção anterior (Figura 2 L). </li><li> Repita 2.9 e 2.10 do lado oposto. </li><li> Agarrar a base do tubo do intestino e puxar anteriormente para remover o esqueleto e intestino tubo branquial (Figura 2 M - N). </li><li> Separa-se o tubo do intestino posterior, fazendo um corte perpendicular ao final do quinto ceratobranquial (Figura 2O </strong&gt;). </li><li> Depois de remover quaisquer fragmentos de osso restantes da caixa craniana do lado dorsal do esqueleto branquial, inserir uma tesoura para o cesto branquial para fazer um corte dorsal (corte anterior para posterior) entre os conjuntos bilaterais de placas dorsal do dente (Figura 3A - D). Certifique-se de corte é centrada para evitar danificar as placas dorsal dente. </li><li> Fazer dois cortes laterais rasa no lúmen do intestino de borracha na extremidade posterior do esqueleto branquial (extremidade anterior do tubo do intestino) para ajudar na abertura do esqueleto branquial (Figura 3E). </li><li> Coloque todos os peixes e pedaços de tecido para um frasco e colocar o esqueleto branquial para um tubo de microcentrífuga com 50% de glicerol, 0,25% de KOH para continuar a limpeza suave, ou 100% de glicerol, se não mais de compensação é necessário. frascos de etiquetas e tubos com um identificador único para que eles possam ser rastreados. A quantidade de purificação necessário é em grande parte uma função do tamanho do peixe, peixe adulto grande (mais de 40 mm de comprimento padrão) normalmente exigem compensação adicional. </li></ol><img alt="Figura 2" src="/files/ftp_upload/54056/54056fig2.jpg" /> Figura 2:. Stickleback branquial esqueleto dissecção Alizarina Red manchado peixes Gasterosteus aculeatus pronto para dissecção. O olho é despigmentada da extensa clareira. As setas azuis indicam a direcção do movimento. (A) Vista lateral da cabeça stickleback, anterior está à direita. (B) A remoção de membrana que cobre o olho. (C) A remoção do olho. (D) Dorsal corte acima do opérculo. Corte ósseo (E) frontal. (F) parasphenoide corte. (G - I) A remoção do esqueleto facial. (J) A remoção do esqueleto branquial conexões de tecidos moles ventral. (K - L) Remoção de dorsais conexões esqueleto branquial. (&lt;strong&gt; M - N) A remoção do esqueleto branquial. (O) Separa-se o tubo digestivo do esqueleto branquial. Veja os passos 2.1 a 2.16 para mais detalhes. Barra de escala = 5 mm. <a href="https://www.jove.com/files/ftp_upload/54056/54056fig2large.jpg" target="_blank">Por favor clique aqui para ver uma versão maior desta figura.</a> 3. branquial esqueleto Re-coloração (se necessário) <ol><li> Para mancha mais escura do esqueleto branquial ou tecido mais clara, remover glicerol a 50%, solução de KOH 0,25% e lava-se com KOH a 1%, duas vezes (uma lavagem de cinco minutos, seguida por uma segunda lavagem 24 h, agitando horizontalmente num agitador de plataforma). </li><li> Retirar 1% de KOH e re-mancha com 0.008% vermelho de alizarina S em 1% de KOH durante 24 h. </li><li> Remover manchas e substituir com 1% de KOH durante 24 h. </li><li> Remoção da solução de KOH e substituir com 50% de glicerol, 0,25% KOH. </li></ol> 4. Montagem branquial Skeleton <ol><li> Remover esqueleto branquiala partir de 50% de glicerol, 0,25% de KOH ou 100% de glicerol e local perto da parte inferior de um x 60 milímetros lamela de vidro com 22 milímetros lado dorsal voltada para cima (Figura 3F). Adicionam-se algumas gotas de 50% de glicerol, 0,25% de KOH ou 100% de glicerol em cima de esqueleto branquial. Se a transição a partir de 50% de glicerol, 0,25% de KOH e 100% de glicerol, solução mudança em um tubo de microcentrífuga e agitar durante&gt; 5 min antes da montagem para equilibrar tecido. </li><li> Rolar para fora duas pequenas bolas de massa de modelar e colocar em cada extremidade da lâmina de cobertura para agir como espaçadores. </li><li> Vagamente colocar uma segunda lamela por cima com pressão suficiente para achatar o esqueleto branquial anterior (Figura 3G). </li><li> Peel abrir a aba dorsal esquerda, incluindo placas de dentes dorsais, alise, e deslize entre as lamelas (Figura 3h). </li><li> Técnica Repita com a aba dorsal direita e empurrar toda esqueleto branquial longe da borda da lamela (Figura 3I). <ol><li> Alterarnativamente, segure ambas as abas abertas dorsais com uma pinça e coloque cuidadosamente a lamela na, achatando o esqueleto branquial em um movimento suave. </li><li> Alternativamente, montar o esqueleto branquial de cabeça para baixo em uma lamela, splaying cada lado dorsal lateralmente assim que a gravidade não permite que o esqueleto branquial para fechar volta. Em seguida, cubra com o segundo x 60 milímetros lamela de vidro 22 mm e inverter prep. Nota: Diferentes técnicas de montagem tendem a trabalhar melhor ou pior para cada indivíduo. Tente cada um e ver o que se sente mais confortável. </li></ol></li><li> Pressione levemente na lamela superior para achatar bolas de argila suficiente para manter o esqueleto branquial montado plana, mas tome cuidado para não esmagar o espécime. <ol><li> Durante o processo de montagem, ceratobranchials pode girar e obscurecer uma fileira de rastros. Remediar esta situação através de pinça entre as lamelas e re-orientar o ceratobranchials ou toda esqueleto branquial deslizante. </li></ol></li><li> Loja prepara apartamento em bandejas de slides no rotemperatura om. Montada em 100% de glicerol, preps pode ser armazenada entre lamelas em ponte por pelo menos uma década. forceps limpas e tesouras com isopropanol ou etanol e dicas de cobertura. </li></ol><img alt="Figura 3" src="/files/ftp_upload/54056/54056fig3.jpg" /> Figura 3:. Plano de montagem do esqueleto branquial Manipulação e montagem do esqueleto branquial é mostrado. As setas azuis indicam a direcção do movimento. Lado para cima (A) branquial esqueleto dorsal. (B - D) Rotação e incisão entre as placas dorsal dente. (E) corte lateral em tecido mole para abrir ainda mais a base do tubo digestivo. Esqueleto (F) Branquial colocado na parte inferior de uma lamela pronto para montagem. (L) Em segundo lugar lamela colocada na metade anterior do esqueleto branquial (acima placas dentárias dorsais). (H - I)montagem plana do esqueleto branquial abrindo abas placa dorsal dente e deslizando entre duas lamelas. Veja os passos 4.1 até 4.6 para obter mais detalhes. Barra de escala = 5 mm. <a href="https://www.jove.com/files/ftp_upload/54056/54056fig3large.jpg" target="_blank">Por favor clique aqui para ver uma versão maior desta figura.</a>

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J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=An+ancient+gene+network+is+co-opted+for+teeth+on+old+and+new+jaws.">An ancient gene network is co-opted for teeth on old and new jaws.</a> PLoS Biol. 7 (2), e1000031 (2009).</li><li>Stock, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Zebrafish+dentition+in+comparative+context.">Zebrafish dentition in comparative context.</a> J. Exp. Zool. B. Mol. Dev. Evol. 308, 523-549 (2007).</li><li>Liem, K., Greenwood, P. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+functional+approach+to+the+phylogeny+of+the+pharyngognath+teleosts.">A functional approach to the phylogeny of the pharyngognath teleosts.</a> Am. Zool. 21 (1), 83-101 (1981).</li><li>Anker, G. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Morphology+and+kinetics+of+the+head+of+the+stickleback,+Gasterosteus+aculeatus.">Morphology and kinetics of the head of the stickleback, Gasterosteus aculeatus.</a> Trans. Zool. Soc. London. 32 (5), 311-416 (1974).</li><li>Meyer, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Morphometrics+and+allometry+in+the+trophically+polymorphic+cichlid+fish,+Cichlusomu+citrinelfum:+Alternative+adaptations+and+ontogenetic+changes+in+shape.">Morphometrics and allometry in the trophically polymorphic cichlid fish, Cichlusomu citrinelfum: Alternative adaptations and ontogenetic changes in shape.</a> J. Zool., Lond. 221, 237-260 (1990).</li><li>Huysseune, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Phenotypic+plasticity+in+the+lower+pharyngeal+jaw+dentition+of+Astatoreochromis+alluaudi+(Teleostei:+Cichlidae).">Phenotypic plasticity in the lower pharyngeal jaw dentition of Astatoreochromis alluaudi (Teleostei: Cichlidae).</a> Arch. Oral Biol. 40 (11), 1005-1014 (1995).</li><li>Muschick, M., Indermaur, A., Salzburger, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Convergent+Evolution+within+an+adaptive+radiation+of+cichlid+fishes.">Convergent Evolution within an adaptive radiation of cichlid fishes.</a> Curr. Biol. 22 (24), 2362-2368 (2012).</li><li>Cleves, P. A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Evolved+tooth+gain+in+sticklebacks+is+associated+with+a+cis-regulatory+allele+of+Bmp6.">Evolved tooth gain in sticklebacks is associated with a cis-regulatory allele of Bmp6.</a> Proc. Natl. Acad. Sci. 111 (38), 13912-13917 (2014).</li><li>Ellis, N. A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Distinct+developmental+and+genetic+mechanisms+underlie+convergently+evolved+tooth+gain+in+sticklebacks.">Distinct developmental and genetic mechanisms underlie convergently evolved tooth gain in sticklebacks.</a> Development. (142), 2442-2451 (2015).</li><li>Tucker, A. S., Fraser, G. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Evolution+and+developmental+diversity+of+tooth+regeneration.">Evolution and developmental diversity of tooth regeneration.</a> Semin. Cell Dev. Biol. 25-26, 71-80 (2014).</li><li>Erickson, P. A., Glazer, A. M., Cleves, P. A., Smith, A. S., Miller, C. T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Two+developmentally+temporal+quantitative+trait+loci+underlie+convergent+evolution+of+increased+branchial+bone+length+in+sticklebacks.">Two developmentally temporal quantitative trait loci underlie convergent evolution of increased branchial bone length in sticklebacks.</a> Proc. R. Soc. B. 281, (2014).</li><li>Leary, S., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> AVMA Guidelines for the Euthanasia of Animals. , (2013).</li><li>Bell, M. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Evolutionary+phenetics+and+genetics.">Evolutionary phenetics and genetics.</a> Evol. Genet. Fishes. , 431-528 (1984).</li><li>Taylor, W. R., Van Dyke, G. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Revised+procedures+for+staining+and+clearing+small+fishes+and+other+vertebrates+for+bone+and+cartilage+study.">Revised procedures for staining and clearing small fishes and other vertebrates for bone and cartilage study.</a> Cybium. 9 (2), 107-119 (1985).</li><li>Erickson, P. A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+190+base+pair,+TGF-&#946;+responsive+tooth+and+fin+enhancer+is+required+for+stickleback+Bmp6+expression.">A 190 base pair, TGF-&#946; responsive tooth and fin enhancer is required for stickleback Bmp6 expression.</a> Dev. Biol. 401 (2), 310-323 (2015).</li><li>Miller, C. T., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=cis-Regulatory+changes+in+Kit+ligand+expression+and+parallel+evolution+of+pigmentation+in+sticklebacks+and+humans.">cis-Regulatory changes in Kit ligand expression and parallel evolution of pigmentation in sticklebacks and humans.</a> Cell. 131 (6), 1179-1189 (2007).</li><li>Aigler, S. R., Jandzik, D., Hatta, K., Uesugi, K., Stock, D. W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Selection+and+constraint+underlie+irreversibility+of+tooth+loss+in+cypriniform+fishes.">Selection and constraint underlie irreversibility of tooth loss in cypriniform fishes.</a> Proc. Natl. Acad. Sci. U. S. A. 111 (21), 7707-7712 (2014).</li><li>Pasco-Viel, E., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Evolutionary+trends+of+the+pharyngeal+dentition+in+Cypriniformes+(Actinopterygii+Ostariophysi).">Evolutionary trends of the pharyngeal dentition in Cypriniformes (Actinopterygii Ostariophysi).</a> PLoS One. 5 (6), e11293 (2010).</li></ol>

The authors have nothing to disclose.

The branchial skeleton is a complex set of bones in the throat of a fish that manipulates, filters, and masticates food items on their way to the esophagus. Many interesting trophic traits including the patterning of gill rakers, pharyngeal teeth, and branchial bones vary across and within species. The majority of these traits are difficult to near impossible to accurately measure with the branchial skeleton in situ (e.g., gill raker length, branchial bone length). This flat-mounting protocol places all...

Uma incrível quantidade de diversidade existe na cabeça do esqueleto entre os vertebrados, especialmente entre os peixes. Em muitos casos, essa diversidade facilita diferentes estratégias de alimentação 1-4, e pode envolver grandes alterações tanto padronização craniofacial externo e interno. O esqueleto branquial está localizado internamente na garganta de um peixe e rodeia a maior parte da cavidade bucal. O esqueleto branquial é composta por 5 segmentos série homóloga, o anterior quatro dos quais suportam as guelras. Juntos, esses cinco segmentos funcionar como uma interface entre o peixe e sua comida 5. Variação em uma infinidade de traços incluindo rakers Gill, dentes da faringe e ossos branquial contribuir para forrageamento eficiente em diferentes tipos de alimentos. Sticklebacks tenham sido submetidos a uma radiação adaptativa após formas oceânicas ancestrais colonizaram lagos de água doce e riachos em todo o hemisfério norte. A mudança na dietade pequeno zooplâncton no oceano para presas maiores em água doce resultou em variação trófica dramática em várias características craniofaciais 6. Enquanto muitos estudos têm-se centrado nas diferenças craniofaciais externas em sticklebacks 7 - 13, importantes alterações craniofaciais evoluir repetidamente no esqueleto branquial interno. A capacidade de criar híbridos férteis entre as populações stickleback morfologicamente distintas proporciona uma excelente oportunidade para mapear a base genética das alterações evoluíram para o esqueleto branquial. Um traço trófica de importância ecológica é a padronização dos rastros branquiais, ossos dérmicos periódicas que revestem as faces anterior e posterior dos ossos branquial e são usados ​​para filtrar presas. Os peixes que normalmente se alimentam de pequenos presas tendem a ter mais tempo e mais densamente Gill espaçadas rakers em comparação com os peixes que se alimentam de presas maiores 14,15. Variação de rastros branquiais tem sido relatada tanto within e entre espécies 14-19, e os aspectos de emalhar raker padronização contribuir para nichos tróficos e de fitness 16. Décadas de pesquisa têm amplamente documentado número branquiais e variação de comprimento em sticklebacks threespine 17 - 21; no entanto, esses estudos geralmente se concentram na primeira linha de rastros branquiais. Um trabalho recente tem mostrado modularidade no controle genético do número branquiais em todo o esqueleto branquial 22,23 e em uma única linha no raker Gill espaçamento 23 e comprimento de 24 destacando a importância de estudar mais de remar um ou uma única raker Gill para entender o base genética do desenvolvimento da redução branquiais. Uma segunda característica trófica de ambos importância ecológica e biomédica é a padronização dos dentes da faringe. Os dentes em peixes pode ser localizada tanto na mandíbula oral e no esqueleto branquial, conhecido como os dentes da faringe. dentes orais são usados ​​principalmente para prey capturar enquanto os dentes da faringe são utilizados para a mastigação e presa manipulação 25-27. Ambos os conjuntos formam através de mecanismos de desenvolvimento compartilhados e são considerados developmentally homólogo 28. Modularidade interessante ocorre pela qual algumas espécies, como o peixe-zebra, a falta dentes da faringe oral e dorsal 29, enquanto outras espécies têm múltiplas ceratobranchials dentadas, pharyngobranchials, e às vezes dentada basihyal e hypobranchials 30. Em sticklebacks, dentes da faringe são encontrados ventrally no quinto ceratobranquial e dorsal sobre a anterior e posterior pharyngobranchials 31. Cinemática sobre alimentação stickleback mostrar a mandíbula oral é utilizado principalmente para a captura de presas e facilitar a alimentação de sucção 9 deixando a mastigação para a mandíbula da faringe. Em ciclídeos, inferior a morfologia da faringe mandíbula varia dramaticamente 32,33 e foi mostrada para ser adaptável e correlacionada com nicho trófico 34. multipopulações de água doce stickleback PLE têm evoluído aumentos dramáticos na faringe ventral número de dentes 23,35,36. Um trabalho recente demonstrou que a base genética do desenvolvimento deste ganho dente evoluído é em grande parte distinta em duas populações derivadas independentemente de sticklebacks de água doce 36. Ao contrário de dentes de mamíferos, peixes regenerar os dentes de forma contínua ao longo da vida adulta 37. Ambas as populações de água doce dentadas elevados previamente descritos têm evoluído uma taxa acelerada substituição de dentes, fornecendo um sistema de vertebrado rara para estudar a base genética de regeneração 36. Uma terceira característica trófica que evoluiu repetidamente no sticklebacks de água doce é mais ossos epibranchial e ceratobranquial, os branquial homólogos arco segmentar da mandíbula superior e inferior, respectivamente 38. Mais longos ossos branquial conferem um cavidade bucal maior e provavelmente são adaptáveis ​​para permitir presas maiores para ser consumed. Além disso, em outros peixes, ossos epibranchial são importantes para a depressão das placas de dentes dorsal da faringe 25. Como rastros branquiais e dentes da faringe, os ossos branquiais são internas e, portanto, difícil de visualizar ou quantificar facilmente. Aqui apresentamos um protocolo detalhado para dissecar e de montagem fixa o esqueleto branquial, permitindo fácil visualização e quantificação de uma variedade de importantes características craniofaciais. Embora este protocolo descreve uma dissecção stickleback, este mesmo método funciona com uma variedade de outros peixes.

<table><tbody><tr><td>Potassium Hydroxide (KOH)</td><td>EMD</td><td>PX1480-1</td><td></td></tr><tr><td>Glycerol</td><td>Sigma-Aldrich</td><td>G7893-4L</td><td></td></tr><tr><td>10% Neutral Buffered Formalin (NBF)</td><td>Azer Scientific</td><td>NBF-4-G</td><td></td></tr><tr><td>Alizarin Red S</td><td>EMD</td><td>AX0485-3</td><td></td></tr><tr><td>Microscope Cover Glasses 22 mm x 60 mm</td><td>VWR</td><td>16004-350</td><td></td></tr><tr><td>100 mm x 10 mm Glass Petri Dish</td><td>Kimble Chase</td><td>23064-10010</td><td>To dissect samples on</td></tr><tr><td>Sylgard 184 Silicone Elastomer Kit</td><td>Ellsworth Adhesives</td><td>184 SIL ELAST KIT 0.5KG</td><td>Can be poured into glass or plastic Petri dishes to make dissecting plates</td></tr><tr><td>Modeling Clay</td><td>Sargent Art</td><td>22-4000</td><td>1 lb cream</td></tr><tr><td>Scintillation Vials (case of 500)</td><td>Wheaton</td><td>986586</td><td>Borosilicate Glass with Screw Cap</td></tr><tr><td>Forceps-Dumont #5 Inox (Biologie tip)</td><td>FST</td><td>11252-20</td><td>Dumostars are an alternative</td></tr><tr><td>Dissecting Scissors&amp;nbsp;</td><td>FST</td><td>15003-08</td><td>Alternate sizes are available depending on size of sample</td></tr><tr><td>Dissecting Microscope</td><td>Leica</td><td>S6E with KL300 LED</td><td>Many other models work nicely, having a flat base helps</td></tr><tr><td>Microcentrifuge Tubes 1.7 ml</td><td>Denville</td><td>C2170</td><td></td></tr><tr><td>Cardboard slide tray</td><td>Fisher</td><td>12-587-10</td><td></td></tr></tbody></table>

dissection and flat-mounting of the threespine stickleback branchial skeleton

The posterior pharyngeal segments of the vertebrate head give rise to the branchial skeleton, the primary site of food processing in fish. The morphology of the fish branchial skeleton is matched to a species' diet. Threespine stickleback fish (Gasterosteus aculeatus) have emerged as a model system to study the genetic and developmental basis of evolved differences in a variety of traits. Marine populations of sticklebacks have repeatedly colonized countless new freshwater lakes and creeks. Adaptation to the new diet in these freshwater environments likely underlies a series of craniofacial changes that have evolved repeatedly in independently derived freshwater populations. These include three major patterning changes to the branchial skeleton: reductions in the number and length of gill raker bones, increases in pharyngeal tooth number, and increased branchial bone lengths. Here we describe a detailed protocol to dissect and flat-mount the internal branchial skeleton in threespine stickleback fish. Dissection of the entire three-dimensional branchial skeleton and mounting it flat into a largely two-dimensional prep allows for the easy visualization and quantification of branchial skeleton morphology. This dissection method is inexpensive, fast, relatively easy, and applicable to a wide variety of fish species. In sticklebacks, this efficient method allows the quantification of skeletal morphology in genetic crosses to map genomic regions controlling craniofacial patterning.

<html> Este protocolo resulta em um esqueleto montado branquial dissecados e plana (Figura 4), ​​onde uma variedade de importantes características tróficas podem ser quantificados. Do ponto de vista dorsal, todas as linhas de rastros branquiais, todas as placas da faringe dente, e quase todos os ossos branquiais podem ser facilmente visualizados e quantificados 22 - 24,35,36,38,42. Vermelho de Alizarina S reage também em uma ou roda...

Watch this Scientific Journal Video about Dissection and Flat-mounting of the Threespine Stickleback Branchial Skeleton at JoVE.com

Dissection and Flat-mounting of the Threespine Stickleback Branchial Skeleton

The branchial skeleton, including gill rakers, pharyngeal teeth, and branchial bones, serves as the primary site of food processing in most fish. Here we describe a protocol to dissect and flat-mount this internal skeleton in threespine sticklebacks. This method is also applicable to a variety of other fish species.

Dissecção e pay-per-montagem do Threespine Stickleback branquial Skeleton

The posterior pharyngeal segments of the vertebrate head give rise to the branchial skeleton, the primary site of food processing in fish. The morphology ...

dissection-flat-mounting-threespine-stickleback-branchial

Research

JoVE Journal

Biology

9.7K visualizações.  University of California, Berkeley. The branchial skeleton, including gill rakers, pharyngeal teeth, and branchial bones, serves as the primary site of food processing in most fish. Here we describe a protocol to dissect and flat-mount this internal skeleton in threespine sticklebacks. This method is also applicable to a variety of other fish species. 

Vídeo: Dissection and Flat-mounting of the Threespine Stickleback Branchial Skeleton

Expression of Fluorescent Proteins in Branchiostoma lanceolatum by mRNA Injection into Unfertilized Oocytes

We report here a robust and efficient protocol for the expression of fluorescent proteins after mRNA injection into unfertilized oocytes of the cephalochordate amphioxus, Branchiostoma lanceolatum. We use constructs for membrane and nuclear targeted mCherry and eGFP that have been modified to accommodate amphioxus codon usage and Kozak consensus sequences. We describe the type of injection needles to be used, the immobilization protocol for the unfertilized oocytes, and the overall injection set-up. This technique generates fluorescently labeled embryos, in which the dynamics of cell behaviors during early development can be analyzed using the latest in vivo imaging strategies. The development of a microinjection technique in this amphioxus species will allow live imaging analyses of cell behaviors in the embryo as well as gene-specific manipulations, including gene overexpression and knockdown. Altogether, this protocol will further consolidate the basal chordate amphioxus as an animal model for addressing questions related to the mechanisms of embryonic development and, more importantly, to their evolution.

Expression of Fluorescent Proteins in Branchiostoma lanceolatum by mRNA Injection into Unfertilized Oocytes

We report here the robust and efficient expression of fluorescent proteins after mRNA injection into unfertilized oocytes of Branchiostoma lanceolatum. The development of the microinjection technique in this basal chordate will pave the way for far-reaching technical innovations in this emerging model system, including in vivo imaging and gene-specific manipulations.

Expressão de proteínas fluorescentes em<em&gt; Branchiostoma lanceolatum</em&gt; Por injecção de mRNA em oócitos não fertilizados

We report here a robust and efficient protocol for the expression of fluorescent proteins after mRNA injection into unfertilized oocytes of the ...

Biologia do Desenvolvimento

Microinjection for Transgenesis and Genome Editing in Threespine Sticklebacks

The threespine stickleback fish has emerged as a powerful system to study the genetic basis of a wide variety of morphological, physiological, and behavioral phenotypes. The remarkably diverse phenotypes that have evolved as marine populations adapt to countless freshwater environments, combined with the ability to cross marine and freshwater forms, provide a rare vertebrate system in which genetics can be used to map genomic regions controlling evolved traits. Excellent genomic resources are now available, facilitating molecular genetic dissection of evolved changes. While mapping experiments generate lists of interesting candidate genes, functional genetic manipulations are required to test the roles of these genes. Gene regulation can be studied with transgenic reporter plasmids and BACs integrated into the genome using the Tol2 transposase system. Functions of specific candidate genes and cis-regulatory elements can be assessed by inducing targeted mutations with TALEN and CRISPR/Cas9 genome editing reagents. All methods require introducing nucleic acids into fertilized one-cell stickleback embryos, a task made challenging by the thick chorion of stickleback embryos and the relatively small and thin blastomere. Here, a detailed protocol for microinjection of nucleic acids into stickleback embryos is described for transgenic and genome editing applications to study gene expression and function, as well as techniques to assess the success of transgenesis and recover stable lines.

Transgenic manipulations and genome editing are critical for functionally testing the roles of genes and cis-regulatory elements. Here a detailed microinjection protocol for the generation of genomic modifications (including Tol2-mediated fluorescent reporter transgene constructs, TALENs, and CRISPRs) is presented for the emergent model fish, the threespine stickleback.

Microinjeção para Transgénese e Genoma Edição na Threespine Sticklebacks

The threespine stickleback fish has emerged as a powerful system to study the genetic basis of a wide variety of morphological, physiological, and ...

Building Finite Element Models to Investigate Zebrafish Jaw Biomechanics

Skeletal morphogenesis occurs through tightly regulated cell behaviors during development; many cell types alter their behavior in response to mechanical strain. Skeletal joints are subjected to dynamic mechanical loading. Finite element analysis (FEA) is a computational method, frequently used in engineering that can predict how a material or structure will respond to mechanical input. By dividing a whole system (in this case the zebrafish jaw skeleton) into a mesh of smaller 'finite elements', FEA can be used to calculate the mechanical response of the structure to external loads. The results can be visualized in many ways including as a 'heat map' showing the position of maximum and minimum principal strains (a positive principal strain indicates tension while a negative indicates compression. The maximum and minimum refer the largest and smallest strain). These can be used to identify which regions of the jaw and therefore which cells are likely to be under particularly high tensional or compressional loads during jaw movement and can therefore be used to identify relationships between mechanical strain and cell behavior. This protocol describes the steps to generate Finite Element models from confocal image data on the musculoskeletal system, using the zebrafish lower jaw as a practical example. The protocol leads the reader through a series of steps: 1) staining of the musculoskeletal components, 2) imaging the musculoskeletal components, 3) building a 3 dimensional (3D) surface, 4) generating a mesh of Finite Elements, 5) solving the FEA and finally 6) validating the results by comparison to real displacements seen in movements of the fish jaw.

Finite Element Analysis is a frequently used tool to investigate the mechanical performance of structures under load. Here we apply its use to modeling the biomechanics of the zebrafish jaw.

Construindo Modelos de Elementos Finitos para investigar Zebrafish Jaw Biomecânica

Skeletal morphogenesis occurs through tightly regulated cell behaviors during development; many cell types alter their behavior in response to mechanical ...

Characterization Of Multi-layered Fish Scales (Atractosteus spatula) Using Nanoindentation, X-ray CT, FTIR, and SEM

The hierarchical architecture of protective biological materials such as mineralized fish scales, gastropod shells, ram&#8217;s horn, antlers, and turtle shells provides unique design principles with potentials for guiding the design of protective materials and systems in the future. Understanding the structure-property relationships for these material systems at the microscale and nanoscale where failure initiates is essential. Currently, experimental techniques such as nanoindentation, X-ray CT, and SEM provide researchers with a way to correlate the mechanical behavior with hierarchical microstructures of these material systems1-6. However, a well-defined standard procedure for specimen preparation of mineralized biomaterials is not currently available. In this study, the methods for probing spatially correlated chemical, structural, and mechanical properties of the multilayered scale of A. spatula using nanoindentation, FTIR, SEM, with energy-dispersive X-ray (EDX) microanalysis, and X-ray CT are presented.

Characterization Of Multi-layered Fish Scales Atractosteus spatula Using Nanoindentation, X-ray CT, FTIR, and SEM

This paper presents the methods used for probing spatially correlated chemical, structural, and mechanical properties of the multilayered scale of Atractosteus spatula (A. spatula) using nanoindentation, Fourier transform infrared (FTIR) spectroscopy, scanning electron microscopy (SEM), and X-ray computed tomography (X-ray CT). The experimental results have been used to investigate the design principles of protective biological materials.

Caracterização de escamas de peixe multi-camadas (<em&gt; Atractosteus espátula</em&gt;) Usando Nanoindentação, X-ray CT, FTIR, e SEM

The hierarchical architecture of protective biological materials such as mineralized fish scales, gastropod shells, ram&#8217;s horn, antlers, and turtle ...

Bioengenharia

Sequential Photo-bleaching to Delineate Single Schwann Cells at the Neuromuscular Junction

Sequential photo-bleaching provides a non-invasive way to label individual SCs at the NMJ. The NMJ is the largest synapse of the mammalian nervous system and has served as guiding model to study synaptic structure and function. In mouse NMJs motor axon terminals form pretzel-like contact sites with muscle fibers. The motor axon and its terminal are sheathed by SCs. Over the past decades, several transgenic mice have been generated to visualize motor neurons and SCs, for example Thy1-XFP1 and Plp-GFP mice2, respectively.
Along motor axons, myelinating axonal SCs are arranged in non-overlapping internodes, separated by nodes of Ranvier, to enable saltatory action potential propagation. In contrast, terminal SCs at the synapse are specialized glial cells, which monitor and promote neurotransmission, digest debris and guide regenerating axons. NMJs are tightly covered by up to half a dozen non-myelinating terminal SCs - these, however, cannot be individually resolved by light microscopy, as they are in direct membrane contact3.
Several approaches exist to individually visualize terminal SCs. None of these are flawless, though. For instance, dye filling, where single cells are impaled with a dye-filled microelectrode, requires destroying a labelled cell before filling a second one. This is not compatible with subsequent time-lapse recordings3. Multi-spectral "Brainbow" labeling of SCs has been achieved by using combinatorial expression of fluorescent proteins4. However, this technique requires combining several transgenes and is limited by the expression pattern of the promoters used. In the future, expression of "photo-switchable" proteins in SCs might be yet another alternative5. Here we present sequential photo-bleaching, where single cells are bleached, and their image obtained by subtraction. We believe that this approach - due to its ease and versatility - represents a lasting addition to the neuroscientist's technology palette, especially as it can be used in vivo and transferred to others cell types, anatomical sites or species6.
In the following protocol, we detail the application of sequential bleaching and subsequent confocal time-lapse microscopy to terminal SCs in triangularis sterni muscle explants. This thin, superficial and easily dissected nerve-muscle preparation7,8 has proven useful for studies of NMJ development, physiology and pathology9. Finally, we explain how the triangularis sterni muscle is prepared after fixation to perform correlated high-resolution confocal imaging, immunohistochemistry or ultrastructural examinations.

Visualizing individual cells in densely packed tissues, such as terminal Schwann cells (SCs) at neuromuscular junctions (NMJs), is challenging. "Sequential photo-bleaching" allows delineating single terminal SCs, for instance in the triangularis sterni muscle explant, a convenient nerve-muscle preparation, where sequential bleaching can be combined with time-lapse imaging and post-hoc immunostainings.

Sequencial de foto-branqueamento de delinear células de Schwann individuais na junção neuromuscular

Sequential photo-bleaching provides a non-invasive way to label individual SCs at the NMJ. The NMJ is the largest synapse of the mammalian nervous system ...

Neurociência

Dissection and Lateral Mounting of Zebrafish Embryos: Analysis of Spinal Cord Development

The zebrafish spinal cord is an effective investigative model for nervous system research for several reasons. First, genetic, transgenic and gene knockdown approaches can be utilized to examine the molecular mechanisms underlying nervous system development. Second, large clutches of developmentally synchronized embryos provide large experimental sample sizes. Third, the optical clarity of the zebrafish embryo permits researchers to visualize progenitor, glial, and neuronal populations. Although zebrafish embryos are transparent, specimen thickness can impede effective microscopic visualization. One reason for this is the tandem development of the spinal cord and overlying somite tissue. Another reason is the large yolk ball, which is still present during periods of early neurogenesis. In this article, we demonstrate microdissection and removal of the yolk in fixed embryos, which allows microscopic visualization while preserving surrounding somite tissue. We also demonstrate semipermanent mounting of zebrafish embryos. This permits observation of neurodevelopment in the dorso-ventral and anterior-posterior axes, as it preserves the three-dimensionality of the tissue.

Developmental processes such as proliferation, patterning, differentiation, and axon guidance can be readily modeled in the zebrafish spinal cord. In this article, we describe a mounting procedure for zebrafish embryos, which optimizes visualization of these events.

Dissecção e montagem lateral de embriões Zebrafish: Análise de Desenvolvimento da Medula Espinhal

The zebrafish spinal cord is an effective investigative model for nervous system research for several reasons. First, genetic, transgenic and gene ...

A 3-D Tail Explant Culture to Study Vertebrate Segmentation in Zebrafish

Vertebrate embryos pattern their major body axis as repetitive somites, the precursors of vertebrae, muscle, and skin. Somites progressively segment from the presomitic mesoderm (PSM) as the tail end of the embryo elongates posteriorly. Somites form with regular periodicity and scale in size. Zebrafish is a popular model organism as it is genetically tractable and has transparent embryos that allow for live imaging. Nevertheless, during somitogenesis, fish embryos are wrapped around a large, rounding yolk. This geometry limits live imaging of PSM tissue in zebrafish embryos, particularly at higher resolutions that require a close objective working distance. Here, we present a flattened 3-D tissue culture method for live imaging of zebrafish tail explants. Tail explants mimic intact embryos by displaying a proportional slowdown of axis elongation and shortening of rostrocaudal somite lengths. We are further able to stall axis elongation speed through explant culture. This, for the first time, enables us to untangle the chemical input of signaling gradients from the mechanistic input of axial elongation. In future studies, this method can be combined with a microfluidic setup to allow time-controlled pharmaceutical perturbations or screening of vertebrate segmentation without any drug penetration concerns.

Here, we present the protocol for 3-D tissue culture of the zebrafish posterior body axis, enabling live study of vertebrate segmentation. This explant model provides control over axis elongation, alteration of morphogen sources, and subcellular resolution tissue-level live imaging.

Uma cultura de explanta de cauda 3D para estudar segmentação de vertebrados em zebrafish

Vertebrate embryos pattern their major body axis as repetitive somites, the precursors of vertebrae, muscle, and skin. Somites progressively segment from ...

Three and Four-Dimensional Visualization and Analysis Approaches to Study Vertebrate Axial Elongation and Segmentation

Somitogenesis is a hallmark of vertebrate embryonic development. For years, researchers have been studying this process in a variety of organisms using a wide range of techniques encompassing ex vivo and in vitro approaches. However, most studies still rely on the analysis of two-dimensional (2D) imaging data, which limits proper evaluation of a developmental process like axial extension and somitogenesis involving highly dynamic interactions in a complex 3D space. Here we describe techniques that allow mouse live imaging acquisition, dataset processing, visualization and analysis in 3D and 4D to study the cells (e.g., neuromesodermal progenitors) involved in these developmental processes. We also provide a step-by-step protocol for optical projection tomography and whole-mount immunofluorescence microscopy in mouse embryos (from sample preparation to image acquisition) and show a pipeline that we developed to process and visualize 3D image data. We extend the use of some of these techniques and highlight specific features of different available software (e.g., Fiji/ImageJ, Drishti, Amira and Imaris) that can be used to improve our current understanding of axial extension and somite formation (e.g., 3D reconstructions). Altogether, the techniques here described emphasize the importance of 3D data visualization and analysis in developmental biology, and might help other researchers to better address 3D and 4D image data in the context of vertebrate axial extension and segmentation. Finally, the work also employs novel tools to facilitate teaching vertebrate embryonic development.

Here, we describe computational tools and methods that allow visualization and analysis of three and four-dimensional image data of mouse embryos in the context of axial elongation and segmentation, obtained by in toto optical projection tomography, and by live imaging and whole-mount immunofluorescence staining using multiphoton microscopy.

Abordagens de visualização e análise tridimensional para estudar alongamento axial de vertebrados e segmentação

Somitogenesis is a hallmark of vertebrate embryonic development. For years, researchers have been studying this process in a variety of organisms using a ...

Stab Wound Injury Model of the Adult Optic Tectum Using Zebrafish and Medaka for the Comparative Analysis of Regenerative Capacity

While zebrafish have a superior capacity to regenerate their central nervous system (CNS), medaka has a lower CNS regenerative capacity. A brain injury model was developed in the adult optic tectum of zebrafish and medaka and comparative histological and molecular analyses were performed to elucidate the molecular mechanisms regulating the high regenerative capacity of this tissue across these fish species. Here a stab wound injury model is presented for the adult optic tectum using a needle and histological analyses for proliferation and differentiation of the neural stem cells (NSCs). A needle was manually inserted into the central region of the optic tectum, and then the fish were intracardially perfused, and their brains were dissected. These tissues were then cryosectioned and evaluated using immunostaining against the appropriate NSC proliferation and differentiation markers. This tectum injury model provides robust and reproducible results in both zebrafish and medaka, allowing for comparing NSC responses after injury. This method is available for small teleosts, including zebrafish, medaka, and African killifish, and enables us to compare their regenerative capacity and investigate unique molecular mechanisms.

A mechanical brain injury model in the adult zebrafish is described to investigate the molecular mechanisms regulating their high regenerative capacity. The method explains to create a stab wound injury in the optic tectum of multiple species of small fish to evaluate the regenerative responses using fluorescent immunostaining.

Modelo de Lesão por Arma Branca do Adulto Óptico Utilizando Zebrafish e Medaka para Análise Comparativa da Capacidade Regenerativa

While zebrafish have a superior capacity to regenerate their central nervous system (CNS), medaka has a lower CNS regenerative capacity. A brain injury ...

Flat Mount Preparation for Observation and Analysis of Zebrafish Embryo Specimens Stained by Whole Mount In situ Hybridization

The zebrafish embryo is now commonly used for basic and biomedical research to investigate the genetic control of developmental processes and to model congenital abnormalities. During the first day of life, the zebrafish embryo progresses through many developmental stages including fertilization, cleavage, gastrulation, segmentation, and the organogenesis of structures such as the kidney, heart, and central nervous system. The anatomy of a young zebrafish embryo presents several challenges for the visualization and analysis of the tissues involved in many of these events because the embryo develops in association with a round yolk mass. Thus, for accurate analysis and imaging of experimental phenotypes in fixed embryonic specimens between the tailbud and 20 somite stage (10 and 19 hours post fertilization (hpf), respectively), such as those stained using whole mount in situ hybridization (WISH), it is often desirable to remove the embryo from the yolk ball and to position it flat on a glass slide. However, performing a flat mount procedure can be tedious. Therefore, successful and efficient flat mount preparation is greatly facilitated through the visual demonstration of the dissection technique, and also helped by using reagents that assist in optimal tissue handling. Here, we provide our WISH protocol for one or two-color detection of gene expression in the zebrafish embryo, and demonstrate how the flat mounting procedure can be performed on this example of a stained fixed specimen. This flat mounting protocol is broadly applicable to the study of many embryonic structures that emerge during early zebrafish development, and can be implemented in conjunction with other staining methods performed on fixed embryo samples.

Flat Mount Preparation for Observation and Analysis of Zebrafish Embryo Specimens Stained by Whole Mount In situ Hybridization

The zebrafish embryo is an excellent model for developmental biology research. During embryogenesis, zebrafish develop with a yolk mass, which presents three-dimensional challenges for sample observation and analysis. This protocol describes how to create two-dimensional flat mount preparations of whole mount in situ (WISH) stained zebrafish embryo specimens.

Monte Preparação Plano de observação e análise de amostras de embriões Zebrafish manchado por inteiro Monte<em&gt; Em situ</em&gt; Hibridização

The zebrafish embryo is now commonly used for basic and biomedical research to investigate the genetic control of developmental processes and to model ...

Dissecção e pay-per-montagem do Threespine Stickleback branquial Skeleton

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