We appreciate and would like to thank the Howard Hughes Medical Institute for the HHMI Professor award to U.B. which made this project possible. We thank the college at the University of California, Los Angeles for providing facilities and teaching infrastructure support for this work. The work was also supported with funding from Midwestern University and a generous donation from the Charity Fidelity Gift Fund. We thank John VandenBrooks for comments on the manuscript and Krista Pearman for her technical assistance.

Este procedimiento es un procedimiento de 2 días. Día 1 (2 horas + tiempo de disección) Disección 1. Pupal Disco de ojos <ol><li> Seleccione una pupa para la disección. NOTA: La edad de la pupa para ser diseccionado será determinado por las necesidades experimentales. Sin embargo, si el examen de la morfología celular, esto se hace con frecuencia en 42 horas después de la formación pupario (APF) a 25 ° C, que es la edad de las pupas se muestra en el video. Recoger pupas blanco (considerado APF 0 h) con un pincel mojado y organizar en orden cronológico (basado en el tiempo de recogida) en un nuevo vial de alimentos mosca se mantiene a 25 ° C. Diseccionar las pupas de edad en este mismo orden cronológico para mantener las diferencias de tiempo entre las pupas tan cerca como sea posible. </li><li> Transferir la pupa en una gota de solución salina tamponada con fosfato (PBS, pH 7,4, ver materiales para la receta) en una placa de disección de silicona. </li><li> Mantenga la parte superior de la envoltura pupal con fórceps y perforar y abrir la lporción ower del caso pupal con un par de pinzas cortantes. Retire la pupa de la caja en el agujero recién formado. </li><li> Haga un corte diagonal con unas tijeras, a mediados de tórax, en la pupa. Retire los escombros o transferir la cabeza pupa a una nueva gota de PBS. Limpiar utilizando el tubo del soplador pipeta (ver materiales y Figura 1 para más detalles) y añadir PBS adicional según sea necesario. Asegúrese de que para evitar la deshidratación. </li><li> Agarre firmemente la parte superior de la cabeza de la cutícula pupal con un par de fórceps. Con la punta del tubo del ventilador, presione suavemente en el caso de pupa para extruir el cerebro y otros tejidos, incluyendo los discos de los ojos, fuera del caso de pupa. Asegúrese de evitar el acaparamiento de cualquier tejido dentro de la cutícula. </li><li> Usando el tubo del soplador lleno de PBS, soplar suavemente el tejido corporal grasa y otros residuos fuera de la caja de cabeza para separar claramente e identificar los discos cerebro y los ojos. NOTA: Mantener el cerebro unido a la cabeza de pupa caso permitirá al investigador a utilizar la quecaso del anuncio como un &quot;mango&quot; para la futura manipulación del tejido sin dañar los discos de los ojos o el cerebro. Sin embargo, es común para desalojar el cerebro y los ojos discos de la cabeza y este caso no es perjudicial para el procedimiento general y los resultados. A menudo se requieren múltiples intentos de soplado y empujando para extraer con éxito los discos ojo y el cerebro de la cabeza dentro de la caja de pupa y para que estén claramente separadas de tejido circundante. El más limpio y más uno por separado pueden conseguir los discos de los ojos desde el tejido circundante le ayudará a prevenir el tejido extraño de la fijación de los discos de los ojos. </li><li> Después de la disección, transferir inmediatamente el tejido a un plato de vidrio 3 y en hielo con 0,5 ml de solución de Fix (ver Materiales). Flotador el tejido en la superficie de la solución Fix durante unos minutos (típicamente el tiempo que tarda para diseccionar el siguiente conjunto de discos de ojo). NOTA: Si este no es el primer disco de los ojos para ser diseccionado en esta ronda de la disección, completely sumerja el disco anterior del ojo en la solución de Fix. Si la realización de procedimientos de tinción especiales (por ejemplo, especies reactivas del oxígeno, los lisosomas, etc.) esto se debe hacer antes de la fijación. Con el fin de hacer esto, almacenar los discos de los ojos disecados en PBS enfriado con hielo antes de continuar con el protocolo de tinción apropiada. </li><li> Después de la disección y la inmersión de todos los discos ojo que está siendo diseccionado, mover el plato de cristal 3 bien a un eje de balancín y el rock a temperatura ambiente durante 30 min. </li></ol> 2. La inmunotinción <ol><li> Retire con cuidado la solución Fix y añadir 0,5 ml de PBS con 0,3% Triton X-100 (0,3% PBT, ver materiales) y lavar el tejido en una mecedora durante 10 minutos. Repita este paso tres veces más para un total de 4 lavados (10 minutos cada uno). NOTA: la eliminación cuidadosa de la solución desde el pozo se puede realizar bajo un microscopio de disección para evitar daños en los tejidos o pérdida. La solución se puede aspiró cuidadosamente con una pipeta; preferimos una multa-tipped, pipeta de transferencia desechable que ha tenido la apertura aplanado para reducir la posibilidad de aspirar el tejido. </li><li> Al final de la cuarta lavado, quitar el lavado y añadir 0,5 ml de solución de bloque (ver materiales) al pocillo e incubar durante 30 min. NOTA: Este período de tiempo puede extenderse de acuerdo a sus necesidades. </li><li> Al final del tiempo de bloque de 30 min, la pipeta 10 l de solución de anticuerpo primario (diluido en solución de Bloque) en el número apropiado de pocillos en una placa de micropocillos. NOTA: Un pocillo de una microplaca acomodará alrededor de 4 pares de discos de los ojos conectados con el caso de pupa o 8 pares aislados de los discos de los ojos con cerebros conectados. Los anticuerpos primarios utilizados en este protocolo para los datos representativos son anti-fosfotirosina (dilución 1: 500) y anti-Cut (dilución 1: 200). </li><li> Transferir el tejido diseccionado en los pocillos de la placa de micro pozos llenos de la solución de anticuerpo primario desde el plato de cristal 3 también. </li><li> Lugarla microplaca sobre una toalla de papel humedecida (para evitar la deshidratación) en una caja de pipeta vacía punta (u otro recipiente similar) y se almacena a 4 ° C durante la noche. </li></ol> Día 2 (4 horas + tiempo de montaje) <ol start="6"><li> Transferir el tejido de la microplaca a un nuevo plato de cristal 3 bien con 0,3% PBT (≈0.5 ml) y se lava el tejido durante 10 minutos en el balancín. Repita este paso tres veces más para un total de 4 lavados (10 minutos cada uno) </li><li> Retire el último lavado y añadir 0,5 ml de solución Bloquear al pozo. Bloquear durante 30 minutos. NOTA: Este período de tiempo puede extenderse de acuerdo a sus necesidades. </li><li> Eliminar la solución de bloqueo y añadir 0,5 ml de la solución de anticuerpos secundaria (hecha a partir de anticuerpos marcados con fluorescencia adecuadas para su anticuerpo primario y longitud de onda fluorescente, diluido en solución de Block) para el bienestar y proteger el plato de vidrio 3 y de la luz con una cubierta o aluminio papel de aluminio y se incuba durante al menos 2 horas en la sala detemperatura. NOTA: Todos los pasos subsiguientes deben ser protegidos de manera similar de exposición a la luz. Esta incubación se puede extender a toda la noche a 4 ° C, en una configuración similar a la incubación primaria de anticuerpos, pero también se puede realizar en un plato de vidrio 3 y cubierta con la película de laboratorio, o una placa de micropocillos si se desea la conservación de anticuerpos. </li><li> Al final de la incubación del anticuerpo, retire la solución de anticuerpo secundario y añadir 0,5 ml de 0,3% de PBT para el bien y lavar en el rockero de 10 min. Repita este paso para un total de 4 lavados (10 minutos cada uno). NOTA: Si se desea tinción DAPI, antes de comenzar el primer lavado, añadir 0,5 l de solución de DAPI Stock (ver Materiales) a los 500 l de PBT que se utilizarán para el primer lavado (1: 1000 dilución). </li></ol> 3. Montaje <ol><li> Al final de la última de lavado, montar los discos antenales / ojo en una diapositiva utilizando 70% de glicerol o PBS como un medio para eliminar el brain y otros tejidos no deseados en una piscina en un lado de la diapositiva. </li><li> Mover con cuidado el tejido utilizando la presión hidrostática entre las pinzas, o muy suavemente con una punta de pinzas, y la línea de los discos de los ojos en una columna hacia el centro de la diapositiva. </li><li> Eliminar todo glicerol extraña o PBS de todo el tejido (utilizando acción de mecha de un laboratorio toallita o los fórceps trabajar para esto). </li><li> Colocar una pequeña cantidad (≈10 l) de medio de montaje a lo largo de un lado de la columna de ojo de disco y colocar un cubreobjetos sobre el tejido a fin de repartir el medio de montaje sobre los discos de los ojos. </li><li> Deje reposar de diapositivas durante 1 a 2 minutos para permitir que el medio de tejido / montaje para moverse por completo. </li><li> Limpie cualquier medio de montaje adicional de descanso de alrededor de los bordes del cubreobjetos y sellarlo con esmalte de uñas transparente. </li><li> Captura imágenes fluorescentes de los discos de los ojos utilizando microscopía confocal. </li></ol>

<ol>
	<li>Ready, D. F., Hanson, T. E., Benzer, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Development+of+the+Drosophila+retina,+a+neurocrystalline+lattice.">Development of the Drosophila retina, a neurocrystalline lattice.</a> Dev Biol. 53 (2), 217-240 (1976).</li><li>Wolff, T., Ready, D. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+beginning+of+pattern+formation+in+the+Drosophila+compound+eye:+the+morphogenetic+furrow+and+the+second+mitotic+wave.">The beginning of pattern formation in the Drosophila compound eye: the morphogenetic furrow and the second mitotic wave.</a> Development. 113 (3), 841-850 (1991).</li><li>Carthew, R. W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Pattern+formation+in+the+Drosophila+eye.">Pattern formation in the Drosophila eye.</a> Curr Opin Genet Dev. 17 (4), 309-313 (2007).</li><li>Bao, S., Cagan, R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Preferential+adhesion+mediated+by+Hibris+and+Roughest+regulates+morphogenesis+and+patterning+in+the+Drosophila+eye.">Preferential adhesion mediated by Hibris and Roughest regulates morphogenesis and patterning in the Drosophila eye.</a> Dev cell. 8 (6), 925-935 (2005).</li><li>Grzeschik, N. A., Knust, E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=IrreC/rst-mediated+cell+sorting+during+Drosophila+pupal+eye+development+depends+on+proper+localisation+of+DE-cadherin.">IrreC/rst-mediated cell sorting during Drosophila pupal eye development depends on proper localisation of DE-cadherin.</a> Development. 132 (9), 2035-2045 (2005).</li><li>Sprecher, S. G., Desplan, C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Switch+of+rhodopsin+expression+in+terminally+differentiated+Drosophila+sensory+neurons.">Switch of rhodopsin expression in terminally differentiated Drosophila sensory neurons.</a> Nature. 454 (7203), 533-537 (2008).</li><li>Zuker, C. S., Cowman, A. F., Rubin, G. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Isolation+and+structure+of+a+rhodopsin+gene+from+D.+melanogaster.">Isolation and structure of a rhodopsin gene from D. melanogaster.</a> Cell. 40 (4), 851-858 (1985).</li><li>Voas, M. G., Rebay, I. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Signal+integration+during+development:+insights+from+the+Drosophila+eye.">Signal integration during development: insights from the Drosophila eye.</a> Dev Dyn. 229 (1), 162-175 (2004).</li><li>Hsiao, H. Y., 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=Dissection+and+immunohistochemistry+of+larval,+pupal+and+adult+Drosophila+retinas.">Dissection and immunohistochemistry of larval, pupal and adult Drosophila retinas.</a> J Vis Exp. , 4347 (2012).</li><li>Call, G. B., 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=Genomewide+clonal+analysis+of+lethal+mutations+in+the+Drosophila+melanogaster+eye:+comparison+of+the+X+chromosome+and+autosomes.">Genomewide clonal analysis of lethal mutations in the Drosophila melanogaster eye: comparison of the X chromosome and autosomes.</a> Genetics. 177 (2), 689-697 (2007).</li><li>Chen, 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=Discovery-based+science+education:+functional+genomic+dissection+in+Drosophila+by+undergraduate+researchers.">Discovery-based science education: functional genomic dissection in Drosophila by undergraduate researchers.</a> PLoS Biol. 3 (2), 59 (2005).</li><li>Wolff, T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Dissection+techniques+for+pupal+and+larval+Drosophila+eyes.">Dissection techniques for pupal and larval Drosophila eyes.</a> CSH Protoc. 2007, (2007).</li><li>Williamson, W. R., Hiesinger, P. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Preparation+of+developing+and+adult+Drosophila+brains+and+retinae+for+live+imaging.">Preparation of developing and adult Drosophila brains and retinae for live imaging.</a> J Vis Exp. 37, 1936 (2010).</li><li>Xu, T., Rubin, G. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Analysis+of+genetic+mosaics+in+developing+and+adult+Drosophila+tissues.">Analysis of genetic mosaics in developing and adult Drosophila tissues.</a> Development. 117 (4), 1223-1237 (1993).</li><li>Duffy, J. B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=GAL4+system+in+Drosophila:+a+fly+geneticist's+Swiss+army+knife.">GAL4 system in Drosophila: a fly geneticist's Swiss army knife.</a> Genesis. 34 (1-2), 1-15 (2002).</li></ol>

The authors have nothing to disclose.

While it appears that the process is simple and easy to perform, in reality, this technique requires a great deal of practice to master. Routinely, we start students off by learning to dissect and mount third instar eye discs12, which are much easier to work with. This practice helps to develop an appropriate dissection position of the arms, hands and fingers13 so that manipulation of the forceps under the dissecting microscope is stable, easy and experienced. In essence, the practice period shou...

Los campos de la biología celular y del desarrollo se han visto afectados en gran medida por el organismo modelo: Drosophila melanogaster. Dentro de este modelo, los estudios sobre el ojo disco han contribuido en gran medida de los conocimientos relativos a la señalización, la biología celular y otras áreas. El tercer disco ojo estadio larval tarde se ha estudiado ampliamente y es un modelo de gran alcance de utilizar, ya que da una instantánea de una serie de períodos de desarrollo, cada uno con sus propias moléculas y procesos de señalización único, como la morfogénesis surco progresa a través del disco ojo 8. Sin embargo, hay una necesidad de ampliar aún más nuestra comprensión de los procesos de desarrollo en la fase de pupa de desarrollo. Si bien se han realizado estudios sobre el disco de ojo de pupa 3-7, nuestro conocimiento no se acerca a la amplitud del trabajo que se ha realizado en el tercer disco de ojo estadio. Esto es debido, en parte, a la mayor dificultad en la disección de ojo disco de pupa. Por lo tanto, una presentación de lamétodo apropiado de disección podría ampliar en gran medida la investigación en esta área. Mientras que hay etapas en el desarrollo del disco ojo de pupa que son fácilmente disecados, especialmente en torno al período de mediados de pupa, otros períodos de tiempo son mucho más difícil de diseccionar. Este protocolo representa un método para la disección de los discos de los ojos de pupas que se pueden utilizar de forma universal para todos los marcos de tiempo de desarrollo de pupas. Este protocolo se puede utilizar como una alternativa a otro protocolo 9 que muestra un método más fácil y más rápido para diseccionar ojo discos a partir de los puntos de tiempo midpupal. Este protocolo fue filmado y desarrollado para capacitar a los estudiantes avanzados de pregrado en el Consorcio de Investigación de Pregrado de la UCLA en Genómica Funcional (URCFG) 10,11 en la técnica de disección del ojo de pupa originalmente. Muchos estudiantes universitarios fueron capaces de utilizar el vídeo y el método para aprender esta técnica difícil.

<table border="0" cellpadding="0" cellspacing="0">
	<tbody>
		<tr>
			<td>Phosphate-buffered saline (PBS, pH 7.4)</td>
			<td></td>
			<td></td>
			<td>80g NaCl, 2g&#160; KCl, 14.4g Na2HPO4, 2.4g KH2PO4, Bring volume to 1 l, adjust the pH to 7.4, autoclave or filter sterilize, dilute to 1X PBS with autoclaved ddH2O before using.</td>
		</tr>
		<tr>
			<td>Triton X-100</td>
			<td>Promega</td>
			<td>H5142</td>
			<td>Caution: Irritant! Wear gloves.</td>
		</tr>
		<tr>
			<td>0.3% PBT</td>
			<td></td>
			<td></td>
			<td>1.5 ml of Triton X-100, 500 ml 1X PBS.</td>
		</tr>
		<tr>
			<td>37% formaldehyde solution</td>
			<td>Fisher Scientific</td>
			<td>F75P1GAL</td>
			<td>Caution: Toxic, probable human carcinogen! Wear gloves.&#160;</td>
		</tr>
		<tr>
			<td>Fix Solution</td>
			<td></td>
			<td></td>
			<td>(&#8776;4% Formaldehyde in PBS) 50 &#956;l of 37% Formaldehyde, 450 &#956;l 1XPBS, make fresh before use</td>
		</tr>
		<tr>
			<td>Normal goat serum</td>
			<td>Rockland antibodies &#38; assays</td>
			<td>B304</td>
			<td>Aliquot in 1 ml volumes and store at -80C</td>
		</tr>
		<tr>
			<td>Block Solution</td>
			<td></td>
			<td></td>
			<td>10% NGS in PBT.&#160; This can be made and stored at 4 &#176;C for a few days prior to use.</td>
		</tr>
		<tr>
			<td>DAPI stock solution</td>
			<td>Life Technologies</td>
			<td>D3571</td>
			<td>For coutnerstaining nuclei. Prepare a 1 mg/ml solution with ddH2O.</td>
		</tr>
		<tr>
			<td>VectaShield Mounting Medium</td>
			<td>Vector Labs</td>
			<td>H-1000</td>
			<td>Mounting medium</td>
		</tr>
		<tr>
			<td>Glycerol</td>
			<td>Sigma</td>
			<td>G5516</td>
			<td>For mounting. Prepare 70% dilution with ddH2O.</td>
		</tr>
		<tr>
			<td colspan="4">Equipment</td>
		</tr>
		<tr>
			<td>Nutating mixer</td>
			<td>VWR</td>
			<td>82007-202</td>
			<td>Used to rock tissue in 3 well glass dish</td>
		</tr>
		<tr>
			<td>SylGard 182 Silicone Elastomer Kit</td>
			<td>Krayden</td>
			<td>NC9897184</td>
			<td>Used to make silicone dissection dish</td>
		</tr>
		<tr>
			<td>Silicone dissecting dish</td>
			<td></td>
			<td></td>
			<td>Mix Sylgard elastomer kit (above) according to directions gently (to avoid bubbles). Pour mixture into Petri dish (any size). Allow SylGard to cure overnight in 37 &#176;C incubator.</td>
		</tr>
		<tr>
			<td>3 well glass dish</td>
			<td>Corning</td>
			<td>7220-85</td>
			<td>The 3 well variety of these are no longer available, this is the 9 well product.</td>
		</tr>
		<tr>
			<td>72 well microwell minitray</td>
			<td>Nunc</td>
			<td>438733</td>
			<td></td>
		</tr>
		<tr>
			<td>Sharp forceps (Dumont #55)</td>
			<td>Fine Science Tools</td>
			<td>11255-20</td>
			<td></td>
		</tr>
		<tr>
			<td><a name="RANGE!A19">Vannas-type Micro Scissors, Straight, 5mm blade</a></td>
			<td>Ted Pella</td>
			<td>1346</td>
			<td></td>
		</tr>
		<tr>
			<td>100 mm Borosilicate glass capillaries</td>
			<td>World Precision Instruments</td>
			<td>1B100-4</td>
			<td>Pull with needle puller to make fine point tip that allows a small stream of PBS to flow.</td>
		</tr>
		<tr>
			<td>Disposable Transfer Pipets, Fine Tip</td>
			<td>Samco Scientific</td>
			<td>231</td>
			<td></td>
		</tr>
		<tr>
			<td colspan="4">Tubing dimensions given are inner diameter (ID) x outer diameter (OD) x wall thickness in inches</td>
		</tr>
		<tr>
			<td>PVC tubing (1/8 x 3/16 x 1/32)</td>
			<td>Nalgene</td>
			<td>8000-0010</td>
			<td rowspan="3">Use these with pulled needle to assemble the blower tube as shown in Figure 2.</td>
		</tr>
		<tr>
			<td>Tygon Silicone tubing (3/32 x 5/32 x 1/32)</td>
			<td>Saint Gobain Performance Plastics</td>
			<td>ABW00004</td>
		</tr>
		<tr>
			<td>Tygon Silicone tubing (1/32 x 3/32 x 1/32)</td>
			<td>Saint Gobain Performance Plastics</td>
			<td>ABW00001</td>
		</tr>
	</tbody>
</table>

dissection and mounting of drosophila pupal eye discs

The Drosophila melanogaster eye disc is a powerful system that can be used to study many different biological processes. It contains approximately 800 separate eye units, termed ommatidia1. Each ommatidium contains eight neuronal photoreceptors that develop from undifferentiated cells following the passage of the morphogenetic furrow in the third larval instar2. Following the sequential differentiation of the photoreceptors, non-neuronal cells develop, including cone and pigment cells, along with mechanosensory bristle cells3. Final differentiation processes, including the structured arrangement of all the ommatidial cell types, programmed cell death of undifferentiated cell types and rhodopsin expression, occurs through the pupal phase4-7. This technique focuses on manipulating the pupal eye disc, providing insight and instruction on how to dissect the eye disc during the pupal phase, which is inherently more difficult to perform than the commonly dissected third instar eye disc. This technique also provides details on immunostaining to allow the visualization of various proteins and other cell components.

Como un ejemplo de la utilización de este protocolo, los resultados que ilustra midpupal (42 hrs APF a 25 ° C) ojo discos immunostained con diferentes anticuerpos se presentan en la Figura 2. Mediante el uso de un anticuerpo dirigido contra los residuos de fosfotirosina, la membrana de las células puede ser observado (Figura 2A). Esto puede ser usado para identificar la disposición regular de las células ommatidial en el ojo pupal después de los procesos de modelado finales que se producen antes d...

Watch this Scientific Journal Video about Dissection and Mounting of Drosophila Pupal Eye Discs at JoVE.com

Dissection and Mounting of Drosophila Pupal Eye Discs

The goal of this technique is to enable researchers to perform dissection, immunostaining and mounting of pupal eye discs from Drosophila melanogaster of any age.

Disección y montaje de<em&gt; Drosophila</em&gt; Pupal discos Eye

The Drosophila melanogaster eye disc is a powerful system that can be used to study many different biological processes.  It contains approximately 800 ...

dissection-and-mounting-of-drosophila-pupal-eye-discs

Research

JoVE Journal

Biology

Dissection and Mounting of Drosophila Pupal Eye Discs

12.1K vistas.  University of California at Los Angeles (UCLA). The goal of this technique is to enable researchers to perform dissection, immunostaining and mounting of pupal eye discs from Drosophila melanogaster of any age.

Video: Dissection and Mounting of Drosophila Pupal Eye Discs

Dissection of Drosophila Ovaries

La disección de los ovarios Drosophila

Investigación

Biología

Dissection of Imaginal Discs from 3rd Instar Drosophila Larvae

This protocol demonstrates the dissection technique used for isolating imaginal discs from drosophila larvae at the 3rd instar stage. Methods for fixing the tissue after saying and removing the wing, leg, and eye discs are demonstrated directly on a microscope slide for subsequent visualization.

La disección de los discos imaginales de 3er estadio las larvas de Drosophila

Drosophila Larval NMJ Dissection

The Drosophila neuromuscular junction (NMJ) is an established model system used for the study of synaptic development and plasticity. The widespread use of the Drosophila motor system is due to its high accessibility. It can be analyzed with single-cell resolution. There are 30 muscles per hemisegment whose arrangement within the peripheral body wall are known. A total of 35 motor neurons attach to these muscles in a pattern that has high fidelity. Using molecular biology and genetics, one can create transgenic animals or mutants. Then, one can study the developmental consequences on the morphology and function of the NMJ. In order to access the NMJ for study, it is necessary to carefully dissect each larva. In this article we demonstrate how to properly dissect Drosophila larvae for study of the NMJ by removing all internal organs while leaving the body wall intact. This technique is suitable to prepare larvae for imaging, immunohistochemistry, or electrophysiology.

This protocol demonstrates how to dissect Drosophila larvae in preparation for immunohistochemistry and/or imaging of the neuromuscular junction.

Drosophila larval NMJ Disección

The Drosophila neuromuscular junction (NMJ) is an established model system used for the study of synaptic development and plasticity. The widespread use ...

Dissection of Oenocytes from Adult Drosophila melanogaster

In Drosophila melanogaster, as in other insects, a waxy layer on the outer surface of the cuticle, composed primarily of hydrocarbon compounds, provides protection against desiccation and other environmental challenges. Several of these cuticular hydrocarbon (CHC) compounds also function as semiochemical signals, and as such mediate pheromonal communications between members of the same species, or in some instances between different species, and influence behavior. Specialized cells referred to as oenocytes are regarded as the primary site for CHC synthesis. However, relatively little is known regarding the involvement of the oenocytes in the regulation of the biosynthetic, transport, and deposition pathways contributing to CHC output. Given the significant role that CHCs play in several aspects of insect biology, including chemical communication, desiccation resistance, and immunity, it is important to gain a greater understanding of the molecular and genetic regulation of CHC production within these specialized cells. The adult oenocytes of D. melanogaster are located within the abdominal integument, and are metamerically arrayed in ribbon-like clusters radiating along the inner cuticular surface of each abdominal segment. In this video article we demonstrate a dissection technique used for the preparation of oenocytes from adult D. melanogaster. Specifically, we provide a detailed step-by-step demonstration of (1) how to fillet prepare an adult Drosophila abdomen, (2) how to identify the oenocytes and discern them from other tissues, and (3) how to remove intact oenocyte clusters from the abdominal integument. A brief experimental illustration of how this preparation can be used to examine the expression of genes involved in hydrocarbon synthesis is included. The dissected preparation demonstrated herein will allow for the detailed molecular and genetic analysis of oenocyte function in the adult fruit fly.

Dissection of Oenocytes from Adult Drosophila melanogaster

In insects, the oenocytes produce cuticular hydrocarbon compounds. These compounds protect against desiccation and facilitate chemical communication. Here we demonstrate a dissection technique used to isolate the oenocytes from adult Drosophila melanogaster, and illustrate how this preparation can be utilized to study genes involved in hydrocarbon synthesis.

La disección de Oenocytes de Adultos Drosophila melanogaster</em

In Drosophila melanogaster, as in other insects, a waxy layer on the outer surface of the cuticle, composed primarily of hydrocarbon compounds, provides ...

Dissection and Staining of Drosophila Larval Ovaries

Many organs depend on stem cells for their development during embryogenesis and for maintenance or repair during adult life. Understanding how stem cells form, and how they interact with their environment is therefore crucial for understanding development, homeostasis and disease. The ovary of the fruit fly Drosophila melanogaster has served as an influential model for the interaction of germ line stem cells (GSCs) with their somatic support cells (niche) 1, 2. The known location of the niche and the GSCs, coupled to the ability to genetically manipulate them, has allowed researchers to elucidate a variety of interactions between stem cells and their niches 3-12.
Despite the wealth of information about mechanisms controlling GSC maintenance and differentiation, relatively little is known about how GSCs and their somatic niches form during development. About 18 somatic niches, whose cellular components include terminal filament and cap cells (Figure 1), form during the third larval instar 13-17. GSCs originate from primordial germ cells (PGCs). PGCs proliferate at early larval stages, but following the formation of the niche a subgroup of PGCs becomes GSCs 7, 16, 18, 19. Together, the somatic niche cells and the GSCs make a functional unit that produces eggs throughout the lifetime of the organism.
Many questions regarding the formation of the GSC unit remain unanswered. Processes such as coordination between precursor cells for niches and stem cell precursors, or the generation of asymmetry within PGCs as they become GSCs, can best be studied in the larva. However, a methodical study of larval ovary development is physically challenging. First, larval ovaries are small. Even at late larval stages they are only 100&mu;m across. In addition, the ovaries are transparent and are embedded in a white fat body. Here we describe a step-by-step protocol for isolating ovaries from late third instar (LL3) Drosophila larvae, followed by staining with fluorescent antibodies. We offer some technical solutions to problems such as locating the ovaries, staining and washing tissues that do not sink, and making sure that antibodies penetrate into the tissue. This protocol can be applied to earlier larval stages and to larval testes as well.

Dissection and Staining of Drosophila Larval Ovaries

How niches and stem cells form during development is an important question with practical implications. In the Drosophila ovary, germ line stem cells and their somatic niches form during larval development. This video demonstrates how to dissect, stain and mount female gonads from late third instar (LL3) Drosophila larvae.

La disección y la tinción de Drosophila Larvas Ovarios

Many organs depend on stem cells for their development during embryogenesis and for maintenance or repair during adult life. Understanding how stem cells ...

Drosophila Pupal Abdomen Immunohistochemistry

The Drosophila pupal abdomen is an established model system for the study of epithelial morphogenesis and the development of sexually dimorphic morphologies 1-3. During pupation, which spans approximately 96 hours (at 25 &deg;C), proliferating populations of imaginal cells replace the larval epidermis to generate the adult abdominal segments. These imaginal cells, born during embryogenesis, exist as lateral pairs of histoblast nests in each abdominal segment of the larvae. Four pairs of histoblast nests give rise to the adult dorsal cuticle (anterior and posterior dorsal nests), the ventral cuticle (ventral nests) and the spiracles associated with each segment (spiracle nests) 4. Upon puparation, these diploid cells (distinguishable by size from the larger polyploid larval epidermal cells- LECs) begin a stereotypical process of proliferation, migration and replacement of the LECs. Various molecular and genetic tools can be employed to investigate the contributions of genetic pathways involved in morphogenesis of the adult abdomen. Ultimate adult phenotypes are typically analyzed following dissection of adult abdominal cuticles. However, investigation of the underlying molecular processes requires immunohistochemical analyses of the pupal epithelium, which present unique challenges. Temporally dynamic morphogenesis and the interactions of two distinct epithelial populations (larval and imaginal) generate a fragile tissue prone to excessive cell loss during dissection and subsequent processing. We have developed methods of dissection, fixation, mounting and imaging of the Drosophila pupal abdominem epithelium for immunohistochemical studies that generate consistent high quality samples suitable for confocal or standard fluorescent microscopy.

Drosophila Pupal Abdomen Immunohistochemistry

Antibody staining of the Drosophila pupae can enhance genetic analyses of adult abdominal developmental genetics. We present our protocol for dissection, fixation and antibody staining of staged Drosophila pupal abdomen.

Drosophila pupa inmunohistoquímica Abdomen

The Drosophila pupal abdomen is an established model system for the study of epithelial morphogenesis and the development of sexually dimorphic ...

Imaging Through the Pupal Case of Drosophila melanogaster

The longstanding use of Drosophila as a model for cell and developmental biology has yielded an array of tools. Together, these techniques have enabled analysis of cell and developmental biology from a variety of methodological angles. Live imaging is an emerging method for observing dynamic cell processes, such as cell division or cell motility. Having isolated mutations in uncharacterized putative cell cycle proteins it became essential to observe mitosis in situ using live imaging. Most live imaging studies in Drosophila have focused on the embryonic stages that are accessible to manipulation and observation because of their small size and optical clarity. However, in these stages the cell cycle is unusual in that it lacks one or both of the gap phases. By contrast, cells of the pupal wing of Drosophila have a typical cell cycle and undergo a period of rapid mitosis spanning about 20 hr of pupal development. It is easy to identify and isolate pupae of the appropriate stage to catch mitosis in situ. Mounting intact pupae provided the best combination of tractability and durability during imaging, allowing experiments to run for several hours with minimal impact on cell and animal viability. The method allows observation of features as small as, or smaller than, fly chromosomes. Adjustment of microscope settings and the details of mounting, allowed extension of the preparation to visualize membrane dynamics of adjacent cells and fluorescently labeled proteins such as tubulin. This method works for all tested fluorescent proteins and can capture submicron scale features over a variety of time scales. While limited to the outer 20 &#181;m of the pupa with a conventional confocal microscope, this approach to observing protein and cellular dynamics in pupal tissues in vivo may be generally useful in the study of cell and developmental biology in these tissues.

Imaging Through the Pupal Case of Drosophila melanogaster

This paper demonstrates the use of a fast scanning confocal microscope to image cell behavior directly through the puparium. By leaving the pupal case intact, this method allows observation and measurement of dynamic cell processes at a stage of Drosophila development that is difficult to study directly.

Imaging A través de la envoltura pupal de<em&gt; Drosophila melanogaster</em

The longstanding use of Drosophila as a model for cell and developmental biology has yielded an array of tools. Together, these techniques have enabled ...

Dissection and Immunostaining of Imaginal Discs from Drosophila melanogaster

A significant portion of post-embryonic development in the fruit fly, Drosophila melanogaster, takes place within a set of sac-like structures called imaginal discs. These discs give rise to a high percentage of adult structures that are found within the adult fly. Here we describe a protocol that has been optimized to recover these discs and prepare them for analysis with antibodies, transcriptional reporters and protein traps. This procedure is best suited for thin tissues like imaginal discs, but can be easily modified for use with thicker tissues such as the larval brain and adult ovary. The written protocol and accompanying video will guide the reader/viewer through the dissection of third instar larvae, fixation of tissue, and treatment of imaginal discs with antibodies. The protocol can be used to dissect imaginal discs from younger first and second instar larvae as well. The advantage of this protocol is that it is relatively short and it has been optimized for the high quality preservation of the dissected tissue. Another advantage is that the fixation procedure that is employed works well with the overwhelming number of antibodies that recognize Drosophila proteins. In our experience, there is a very small number of sensitive antibodies that do not work well with this procedure. In these situations, the remedy appears to be to use an alternate fixation cocktail while continuing to follow the guidelines that we have set forth for the dissection steps and antibody incubations.

Dissection and Immunostaining of Imaginal Discs from Drosophila melanogaster

The adult structures of Drosophila are derived from sac-like structures called imaginal discs. Analysis of these discs provides insight into many developmental processes including tissue determination, compartment boundary establishment, cell proliferation, cell fate specification, and planar cell polarity. This protocol is used to prepare imaginal discs for light/fluorescent microscopy.

La disección y la inmunotinción de imaginal discos de<em&gt; Drosophila melanogaster</em

A significant portion of post-embryonic development in the fruit fly, Drosophila melanogaster, takes place within a set of sac-like structures called ...

Ex vivo Culture of Drosophila Pupal Testis and Single Male Germ-line Cysts: Dissection, Imaging, and Pharmacological Treatment

During spermatogenesis in mammals and in Drosophila melanogaster, male germ cells develop in a series of essential developmental processes. This includes differentiation from a stem cell population, mitotic amplification, and meiosis. In addition, post-meiotic germ cells undergo a dramatic morphological reshaping process as well as a global epigenetic reconfiguration of the germ line chromatin&#8212;the histone-to-protamine switch.
Studying the role of a protein in post-meiotic spermatogenesis using mutagenesis or other genetic tools is often impeded by essential embryonic, pre-meiotic, or meiotic functions of the protein under investigation. The post-meiotic phenotype of a mutant of such a protein could be obscured through an earlier developmental block, or the interpretation of the phenotype could be complicated. The model organism Drosophila melanogaster offers a bypass to this problem: intact testes and even cysts of germ cells dissected from early pupae are able to develop ex vivo in culture medium. Making use of such cultures allows microscopic imaging of living germ cells in testes and of germ-line cysts. Importantly, the cultivated testes and germ cells also become accessible to pharmacological inhibitors, thereby permitting manipulation of enzymatic functions during spermatogenesis, including post-meiotic stages.
The protocol presented describes how to dissect and cultivate pupal testes and germ-line cysts. Information on the development of pupal testes and culture conditions are provided alongside microscope imaging data of live testes and germ-line cysts in culture. We also describe a pharmacological assay to study post-meiotic spermatogenesis, exemplified by an assay targeting the histone-to-protamine switch using the histone acetyltransferase inhibitor anacardic acid. In principle, this cultivation method could be adapted to address many other research questions in pre- and post-meiotic spermatogenesis.

Ex vivo Culture of Drosophila Pupal Testis and Single Male Germ-line Cysts: Dissection, Imaging, and Pharmacological Treatment

This protocol describes the dissection and cultivation of intact testes and germ-line cysts from Drosophila melanogaster pupae. This method allows microscopic observation of spermatogenesis ex vivo. Furthermore, we describe a pharmacological assay of the effect of inhibitors on specific stages of germ-cell development in pupal testes.

Ex vivo Cultura de Drosophila Pupal Testis y individuales masculinos quistes línea germinal: Disección, Imaging y Tratamiento farmacológico

During spermatogenesis in mammals and in Drosophila melanogaster, male germ cells develop in a series of essential developmental processes. This includes ...

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.

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.

La disección y-montaje plana del esqueleto branquial de tres espinas Stickleback

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

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