This work was supported by NIH P20GM103643 to I. Meng.

1. Preparación de las larvas <ol><li> Para analizar una larva deseada para la locomoción o la posición de preferencia, crecer larvas bajo condiciones estándar para la edad deseada para ensayar el uso de alimentos 10 mosca estándar 11. </li><li> Haga un filtro de malla por el estiramiento de nylon de grado serigrafía malla sobre un embudo. Asegure la malla en el cuello de embudo con la goma. Colocar el embudo en un vaso de precipitados. </li><li> Para recoger las larvas para el análisis, scoop una espátula llena de alimentos que contienen larvas alimentándose de la botella de cultivo y lavar con agua del grifo RT sobre el filtro de malla, la recogida de larvas individual directamente de la malla con un pincel 10. </li></ol> 2. Preparación de tubos de ensayo <ol><li> Para preparar para tapar los tubos de ensayo, hervir cuidadosamente un gel de agar al 4% y se vierte en una placa de Petri a una profundidad de 1,5 cm. Esto proporcionará un enchufe para cada lado del tubo cuando está encerrado animal. La solución de 4% es suficientemente densa para evitar que las larvas de penetrating los enchufes. </li><li> Asegúrese de que los tubos estén limpios y claros antes de la inserción de la larva. Si no lo son, esto puede bloquear los movimientos de que se está grabando. </li><li> Para asegurar larvas tienen suficiente humedad para el movimiento, prepare un frasco que contiene una pequeña cantidad de agua caliente. Invierta la botella, orientar cuidadosamente la salida hacia un lavabo y apretar suavemente para expulsar el agua del tubo de recogida. </li><li> Inserte la salida de la botella en el tubo de ensayo. Apriete la botella para entregar vapor de agua en el tubo de ensayo hasta que aparezca una fina capa de condensación en la pared del tubo. Video 1 muestra una larva se mueve en un tubo con una cantidad apropiada de la humedad. </li><li> Para sellar la larva en el tubo, quitar el gel de agar 1,5 cm de espesor de la placa de Petri y colocar sobre una superficie de malla para permitir el flujo de aire por debajo de la agar de modo que un tapón de agar puede ser insertado en el tubo. Presione un extremo del tubo de ensayo en el gel dos veces para insertar dos tapones de gel en un extremo. </li><li> Con un paintbprecipitarse, coloque una larva en el tubo de aproximadamente 1,5 pulgadas de profundidad y sellar el tubo presionando el extremo más cercano a la larva en el gel de agar. La presión resultante forzará a cabo el segundo tapón de gel de agar desde el extremo opuesto y sellar el animal dentro del tubo. </li><li> Colocar los tubos en el dispositivo MB5 Multi-Beam Drosophila Activity Monitor (DAM), y ajustar las posiciones de los tubos para que los animales no pueden ir más allá de la gama de los sensores. </li><li> Para asegurarse de que los tubos de ensayo no se deslizan fuera del marco de lectura de infrarrojos del dispositivo durante el transporte, mantenga el tubo en su lugar mediante la fijación de un anillo de masilla alrededor de cada tubo, donde entra en contacto con el dispositivo de grabación. </li></ol> 3. Medición de la Actividad <ol><li> La actividad de registro en una incubadora para evitar lecturas erróneas que pueden ocurrir debido a las sombras, luces fluorescentes o de las variaciones de temperatura en el laboratorio. Consulte la Figura 5 para un arreglo sugerido del sistema. </li><li> Establecer una incubadora a 20 ° C (ver Figura 1). Para evitar falsas grabaciones debido a la interferencia de fuentes de luz incandescentes durante la grabación, apague las luces fluorescentes de la incubadora y el uso de una fuente de luz LED por separado durante la grabación en la incubadora. Realizar un ensayo sin animales para garantizar que las condiciones de luz no desencadenar aberrante sensores. No debe haber datos de movimiento grabadas después de esta prueba. </li><li> Permita que las larvas se adapte a la configuración de la incubadora 20 ° C durante 5 minutos antes de comenzar el ensayo. </li><li> Para establecer el sistema DAM a intervalos de grabación que desee (por ejemplo, 1 min), asegúrese de software de grabación del sistema DAM se descarga al ordenador central 12 y abrir el archivo del sistema DAM antes de conectar la cámara de grabación a la interfaz Psiu. </li><li> Para ajustar la frecuencia de grabación deseado en el que se guardarán los datos, seleccione las preferencias y haga clic encima o por debajo de la opción intervalo de lectura para seleccionar diferentes marcos de tiempo en el que los datosserá almacenado. Por ejemplo, seleccione la lectura de tiempos de intervalo de 1 segundo a 1 hora. </li><li> Para seleccionar el parámetro que varía para grabar datos, elegir preferencias y luego seleccione las casillas correspondientes en virtud de salida de tipo de datos (cuentas, movimientos, posiciones y habitar, ver Tabla 1). Cada parámetro proporciona un análisis único de la actividad larval dentro del tubo. </li><li> Para iniciar la grabación, conecte el monitor a la unidad de interfaz de fuente de alimentación (Psiu) utilizando cable telefónico CAB6. Conecte el Psiu a una toma de corriente. Una luz verde indicará conexión apropiada. </li><li> Conecte el Psiu a través de un cable de bus serie universal (USB) a un Macintosh o PC con Windows para la grabación de datos. Abra el programa DAM SystemMB1v6x en el equipo para iniciar automáticamente la grabación de datos. </li><li> Después se completa el tiempo de recogida deseada, seleccione Salir y salga ahora en la pantalla de la actividad DAM; los datos se guardará automáticamente bajo DAM de datos del sistema. Tome este archivo de datos (por ejemplo, monitorear 1) y arrastre<html> en una carpeta separada. Esto almacenará los datos en bruto desde el software DAM para que más tarde pueden ser procesados. </li></ol> 4. Preparación de los datos para el procesamiento (DAM FileScan) <ol><li> Para procesar los datos en bruto en un formato comprensible abrir la aplicación DAM FileScan y seleccione Seleccionar carpeta de datos de entrada. A continuación, seleccione la carpeta de datos y el archivo deseado y seleccione la opción de escaneado. Por último, seleccione la longitud bin al período lectura deseada. Esto va a organizar los datos en bruto en los parámetros establecidos por el operador y el programa informará de los datos recogidos en ese rango particular. </li><li> Seleccione el tipo de datos de salida para analizar el ajuste movimiento deseado (recuento del monitor, se mueve, moran). Bajo el menú de lecturas adicionales, seleccione suma a bin (esto es si la longitud bin es mayor que el intervalo de lectura sistema seleccionado). </li><li> Nombre del archivo de manera adecuada y guardar. El archivo se almacena en la misma ubicación que la carpeta del paso 3.9. </li></ol>_title &quot;&gt; 5. Datos Acceso de Análisis <ol><li> Con el fin de recoger promedio mueve, proceso los datos brutos generados desde el paso 4. Para generar una tabla en una hoja de cálculo, abra el archivo que se guardó previamente (paso 4.3), y cuando aparezca la ventana del asistente de importación de texto, seleccione acabado para abrir los archivos de datos en un formato de hoja de cálculo. Nota: Dependiendo del tipo de datos analizados, la hoja de cálculo se leerá de manera diferente. Normalmente para medir movimientos de monitor o recuentos, el período de tiempo del estudio se registró numéricamente, mientras que cada tubo de lectura individual recibirá una carta designado. Cuando la visualización de los datos en la hoja de cálculo, las columnas representan KZ las ranuras para tubos de ensayo 1-16, respectivamente. Las filas representan los puntos de datos recogidos. </li><li> Por ejemplo, si se recogieron mueve durante 20 min en intervalos de 1 min, promediar las 20 filas para calcular un número medio de movimientos / minuto y otras mediciones. </li></ol>

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Science Education Database Available from: <a target="_blank" href="https://www.jove.com/science-education-database/3/essentials-of-biology-1-yeast-drosophila-and-c-elegans">https://www.jove.com/science-education-database/3/essentials-of-biology-1-yeast-drosophila-and-c-elegans</a> (2015)</li><li>Woods, J. K., Kowalski, S., Rogina, B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Determination+of+the+spontaneous+locomotor+activity+in+Drosophila+melanogaster.">Determination of the spontaneous locomotor activity in Drosophila melanogaster.</a> J. Vis. Exp. (86), e51449 (2014).</li><li>Troncoso, B., Godoy-Herrera, R., Waldo, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+development+of+larval+movement+patterns+in+Drosophila).">The development of larval movement patterns in Drosophila).</a> Heredity. 58 (1), 321-329 (1987).</li><li>Helfrich, C., Engelmann, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Circadian+rhythm+of+the+locomotor+activity+in+Drosophila.+melanogaster.and+its+mutants+&#8216;sine+oculis&#8217;+and+&#8216;small+optic+lobes.">Circadian rhythm of the locomotor activity in Drosophila. melanogaster.and its mutants &#8216;sine oculis&#8217; and &#8216;small optic lobes.</a> Physiological Entomology. 8 (3), 257-272 (1983).</li><li>Johnson, A. W., Carder, W. 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The authors declare that they have no competing financial interests.

Actividad de las larvas de Drosophila está influenciada por una variedad de factores incluyendo el genotipo 8, 13 años de edad y la temperatura ambiente 2. Aunque poderosos métodos videográficos capaces de análisis muy detallado han sido desarrollados por los que estudian la locomoción 5, este nivel de detalle puede ser superfluo para aquellos que deseen para determinar los parámetros básicos de la actividad. El método descrito aquí emplea un dispositivo que está disponible en muchos laboratorios, es fácil de operar, genera resultados altamente reproducibles, y es manejable incluso para aquellos cuyo principal foco de investigación no es la locomoción. Los ejemplos de resultados demuestran que este ensayo se puede utilizar para detectar cambios significativos en la motilidad en larvas sometidas a diferentes temperaturas (Figura 1) y de diferentes genotipos (Figura 2). Cuando se midieron las larvas a temperaturas comprendidas entre 5 ° C - 35 ° C, suactividad aumenta con la temperatura, a excepción de un quiebre en la tendencia entre 20 ° C y 25 ° C (Figura 1). Se ha demostrado por Ainsley y compañeros de trabajo que forrajeo larvas de tercer estadio temprano prefieren temperaturas dentro de +/- 2 ° C de la temperatura de 25 ° C típico de cultivo. Sin embargo, cuando las larvas entran vagando mediados tercera fase instar prefieren temperaturas algo más frescas 2. Ese hallazgo es consistente con la observación de que la actividad locomotora para las larvas de tercer estadio es mayor a 20 ° C a 25 ° C, lo que sugiere que una parte de los animales ensayados estaban en la etapa errante y más activa a las temperaturas más frías, y en menor medida en la temperatura de cultivo normal de 25 ° C. Este método ofrece simplicidad, objetividad y robusto rendimiento, pero hay limitaciones. Las aplicaciones descritas anteriormente representan ensayos tienen lugar durante un período de tiempo relativamente corto, en parte debido a que la configuración actual no se prlarvas ovide con una fuente de alimento. Garantizar una nutrición adecuada sería necesario estudiar los cambios en la actividad durante períodos prolongados de tiempo o para medir el ritmo circadiano en el largo plazo. Los tapones de agar 4% pueden restringir el intercambio de gases entre la cámara y el entorno externo, lo que podría resultar en que las larvas experimentando condiciones de hipoxia. Sin embargo, esto no parece afectar a la actividad dentro de un período de ensayo de 20 min, porque cuando se analizaron mueve promedio por minuto de las larvas durante cada minuto de la época, las larvas no parece mostrar ningún cambio en la actividad durante el periodo de grabación (Figura 4) . Debido a que el dispositivo registra continuamente la posición que representa una mejora en la captura de más movimiento en comparación con los métodos no automatizados citados, sin embargo algunos movimiento hace escapar a la detección. Muy pequeños movimientos de los animales no podrían desencadenar una respuesta de este dispositivo, y las larvas se pueden mover de forma circunferencial dentro de una infraestructurahaz rojo sin romper vigas vecinos, dando lugar a lecturas erróneamente bajas. Sin embargo, dado que este tipo de error se espera que se produzca en todos los grupos de tratamiento, es poco probable que cause resultados engañosos. Aunque larvas de tercer estadio son el foco principal de este análisis, el dispositivo es capaz de medir el movimiento de las larvas primero y segundo instar mucho más pequeño, así (Figura 3). Como se esperaba, el número de movimientos registrados por minuto en los animales más jóvenes es menor que la de los animales más grandes tercera fase larval. Aunque la gama de usos para este dispositivo aún no se ha demostrado, hay una variedad de otras adaptaciones que podrían diversificar los usos de este aparato para estudios con larvas. Por ejemplo, el dispositivo permite una medición &#39;permanencia&#39;, que representa el tiempo pasado en una región determinada del tubo. Esto puede proporcionar información valiosa cuando se emplea en diversos Drosophila larval taxis unssays. Al colocar el aparato en su lado de manera que los tubos están orientados verticalmente en lugar de horizontalmente, uno podría medir geotaxis larvales. Para medir fototaxis, un gradiente de luz se pudo establecer en los tubos, probando si las larvas tienen una preferencia por la luz o su ausencia. Para estudiar la quimiotaxis, la sustancia de ensayo podría ser colocado en uno de los tapones de agar y la posición de las larvas podría revelar entonces determinar su preferencia por o la evitación de la sustancia química. El sistema de monitorización permite el análisis de diversos parámetros de movimiento, que se resumen en la Tabla 1. Al seleccionar todos los parámetros durante la configuración pre-ensayo (véase el paso 3.6), el experimentador puede elegir el parámetro a analizar después del ensayo. Sin embargo, si no se ha seleccionado ninguna opción, que los datos no estará disponible para el análisis post hoc. Cabe señalar que después de cada período de tiempo seleccionado, los datos se congelan a los recuentos actuales y guardan en el ordenador anfitrión. La recolección de datos se restablece acero después de este periodo y comienza de nuevo, proporcionando una serie de puntos de datos intervalo de tiempo. Hay que dejar de fumar de forma manual para finalizar la grabación de datos. Los estudios futuros que implican este método se centrará en el uso del parámetro de permanencia y sus diversas aplicaciones. También puede ser posible desarrollar un protocolo que permita que se produzcan estudios durante un período de tiempo más largo, tales como estudios circadianos, por el suministro de alimentos y el intercambio de tapones de agar para un material más permeable a los gases 14. Necesitarían niveles de humedad para ser controlado, así como las condiciones secas inhiben la locomoción 15. Actualmente, este protocolo proporciona un método preciso, simple y rentable para evaluar los parámetros básicos de la actividad de las larvas bajo una variedad de condiciones experimentales.

The use of Drosophila as a genetic tool has transformed scientific knowledge of biological systems. Drosophila larvae have been used in a variety of studies including nociception1, development2 and as a model for the study of human disease genes3. Drosophila activity encompasses a range of behaviors that vary under different conditions including temperatures2, exposure to drugs4 and amongst different genotypes. Yet, despite the significant use of the larva as a model organism, a simple, standardized method to analyze larval activity has not been available. Presently, many larval locomotion studies employ sophisticated video analysis software5. While powerful, the complexity of such automated tools may discourage labs that are not already equipped to study locomotion from including analysis of informative activity parameters in their studies. In other current non-automated methods, such as the grid crawling analysis, motion is scored by a human observer, which introduces the possibility of subjectivity and limits throughput to one animal at a time6-7. A similar study used a 5-lane crawling assay, which measured the time it took larvae to travel a certain linear distance8. In such non-automated assays, displacement is measured but this does not account for non-linear travel between the start and end points. As discussed below, the method described here accounts for more of the actual larval movement, is objective, easy to operate, and offers robust throughput.
To easily study larval activity behavior without the compromise of accuracy, efficiency, or cost, this method employs the TriKinetics Drosophila Activity Monitor (DAM), a device often used to study adult activity. Using one device to study both adult and larval activity is cost-effective, and allows direct comparison of motion by animals at these two life stages. The system, featuring the manufacturer&#8217;s highest level of resolution, makes use of 17 infrared detection beams per assay tube, which record larval activity when sensor beams are broken within the 16 individual tubes. The system then automatically saves recorded information to a computer, making it available for manipulation with basic graphing software. The data obtained represents the beams that were broken by individual larvae (which can be converted into a rate), movement when a larva stays within a detector beam and the position of the animals within the assay chambers during a recording period (allowing one to calculate position preference). The system is efficient and relatively simple to operate, and brings highly reproducible basic activity analysis within the reach of any laboratory studying Drosophila larvae.
To demonstrate the power of this assay, data are presented that show its use to verify differences in activity resulting from varying ambient temperatures, as well as through the comparison of a mutant previously described as hypoactive (iav1)9 with a widely analyzed control (w1118).

<table border="0" cellpadding="0" cellspacing="0">
	<tbody>
		<tr>
			<td>Drosophila Activity Monitor, Multibeam, 16 tubes, including wires</td>
			<td>TriKinetics Inc.&#160;</td>
			<td>MB5</td>
			<td></td>
		</tr>
		<tr>
			<td>Power Supply Interface for Activity Monitor&#160;</td>
			<td>TriKinetics Inc.&#160;</td>
			<td>PSIU24</td>
			<td></td>
		</tr>
		<tr>
			<td>Glass 80 x 5 mm tubes for Activity Monitor (100)</td>
			<td>TriKinetics Inc.&#160;</td>
			<td>PGT 5x80</td>
			<td></td>
		</tr>
		<tr>
			<td>DAMsystemMB1v6x Data Acquisitions Software for Macintonsh OSX (Intel)</td>
			<td><a href="http://www.trikinetics.com/">www.trikinetics.com</a></td>
			<td></td>
			<td>free download</td>
		</tr>
		<tr>
			<td>DAMFileScan 108x software for Macintosh</td>
			<td><a href="http://www.trikinetics.com/">www.trikinetics.com</a></td>
			<td></td>
			<td>free download</td>
		</tr>
		<tr>
			<td>USB software (PSIUdrivers.zip).</td>
			<td><a href="http://www.trikinetics.com/">www.trikinetics.com</a></td>
			<td></td>
			<td>free download</td>
		</tr>
		<tr>
			<td>DAMSystem Notes 308</td>
			<td><a href="http://www.trikinetics.com/">www.trikinetics.com</a></td>
			<td></td>
			<td>free download</td>
		</tr>
		<tr>
			<td>Zeiss Stemi 2000C- Stereo Microscope</td>
			<td>Spectra Services</td>
			<td>SP-STEMI2000C-BS</td>
			<td></td>
		</tr>
		<tr>
			<td>Carbon Dioxide</td>
			<td>Maine Oxy</td>
			<td></td>
			<td>anaesthesia</td>
		</tr>
		<tr>
			<td>Fly Pad</td>
			<td>Genesee</td>
			<td>59-114</td>
			<td>surface for sorting anaesthetized flies</td>
		</tr>
		<tr>
			<td>Small paint brush&#160;</td>
			<td>Winsor &#38; Newton</td>
			<td>#2 ROUND</td>
			<td>or similar, used for sorting anaesthetized flies</td>
		</tr>
		<tr>
			<td>Silk Screen Printing Mesh (160)</td>
			<td>msj-gallery.com</td>
			<td>SM160W63-3YD</td>
			<td>pore sized used in this protocol was ~ 0.1 mm</td>
		</tr>
		<tr>
			<td>Tegosept</td>
			<td>Genesee</td>
			<td>20-258</td>
			<td>preservative</td>
		</tr>
		<tr>
			<td>Ethanol (190proof)</td>
			<td>Pharmco</td>
			<td>111000190</td>
			<td>used to dissolve Tegosept</td>
		</tr>
		<tr>
			<td>6 oz Square Bottom Bottle (PP)</td>
			<td>Genesee</td>
			<td>32-130</td>
			<td></td>
		</tr>
		<tr>
			<td>&#34;Flugs&#34; for Plastic Fly bottles</td>
			<td>Genesee</td>
			<td>49-100</td>
			<td></td>
		</tr>
		<tr>
			<td>Drosophila Vials, Wide (PS)</td>
			<td>Genesee</td>
			<td>32-117</td>
			<td></td>
		</tr>
		<tr>
			<td>Flugs for wide plastic vials</td>
			<td>Genesee</td>
			<td>49-101</td>
			<td></td>
		</tr>
		<tr>
			<td>Yellow Degerminated Corn Meal</td>
			<td>Gold Medal</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Drosophila agar</td>
			<td>LabScientific</td>
			<td>FLY 8020</td>
			<td></td>
		</tr>
		<tr>
			<td>Baker&#39;s Yeast - Red Star</td>
			<td>King Arthur Flour</td>
			<td>1270</td>
			<td></td>
		</tr>
		<tr>
			<td>Granulated Sugar - Extra Fine</td>
			<td>Domino</td>
			<td></td>
			<td></td>
		</tr>
	</tbody>
</table>

measurement of larval activity in the drosophila activity monitor

Drosophila larvae are used in many behavioral studies, yet a simple device for measuring basic parameters of larval activity has not been available. This protocol repurposes an instrument often used to measure adult activity, the TriKinetics Drosophila activity monitor (MB5 Multi-Beam Activity Monitor) to study larval activity. The instrument can monitor the movements of animals in 16 individual 8 cm glass assay tubes, using 17 infrared detection beams per tube. Logging software automatically saves data to a computer, recording parameters such as number of moves, times sensors were triggered, and animals&#8217; positions within the tubes. The data can then be analyzed to represent overall locomotion and/or position preference as well as other measurements. All data are easily accessible and compatible with basic graphing and data manipulation software. This protocol will discuss how to use the apparatus, how to operate the software and how to run a larval activity assay from start to finish.

La Figura 1 muestra los resultados de un estudio de respuesta de la temperatura de control de larvas de tercer instar, 1118 w, utilizando el dispositivo de monitorización para detectar diferencias en la locomoción de larvas en siete diferentes temperaturas. Las larvas se lava y se coloca en el dispositivo de la actividad DAM como se describe anteriormente, y se coloca en una incubadora a la temperatura deseada. A continuación, el aparato se dejó aclimatar al medio ambiente durante 5 minutos antes de que comenzara la grabación. Cada larva fue analizada individualmente para la locomoción en un período de 20 min y el número medio de movimientos por minuto se calculó para cada animal y se promediaron para cada conjunto de 32 animales. Se analizaron los datos y se representan mediante un programa de hoja de cálculo. Las larvas exhibió aumentar significativamente la actividad como la temperatura aumenta correspondientemente 5-35 ° C en incrementos de 5 grados, con excepción de un descanso en esta tendencia a 20 ° C y 25 ° C. Para verificar que las diferencias coudetectarse ld entre un control y un mutante descrito previamente como hipoactivo, larvas inactiva (IAV 1) fueron probados. Los datos se analizaron como se mueve / minuto para cada uno de los 32 animales y se calculó entonces un promedio. Como se muestra en la Figura 2, el análisis indica que las larvas inactivo fueron significativamente menos móvil que un control. Mientras que son mucho más pequeñas que las larvas de tercer estadio, la actividad de primero y segundo estadio las larvas también era medible, como se muestra en la Figura 3. Actividad de larvas de tercer instar en cada minuto del ensayo de 20 min se muestra a permanecer relativamente constante durante todo el período ( la Figura 4). <img alt="Figura 1" src="/files/ftp_upload/52684/52684fig1.jpg" /> Figura 1. w 1118 locomoción larval se registró a temperaturas que varían desde 5 ° C -. 35 ° C Eaccolumna h representa el movimiento promedio de 32 animales tercera instar con jugadas individuales por minuto en promedio, entre el conjunto. * Todos los promedios son significativamente diferentes entre sí excepto 10 ° C y 15 ° C (p = 0,116) (Letras diferentes indican una diferencia significativa, test t de Student). <img alt="Figura 2" src="/files/ftp_upload/52684/52684fig2.jpg" /> Figura 2. Control de larvas de tercer estadio en comparación con (iav 1) larvas inactiva a 20 ° C. Iav 1 larvas exhiben significativamente menos movilidad en comparación con el control. <img alt="Figura 3" src="/files/ftp_upload/52684/52684fig3.jpg" /> Figura 3. Medición de la actividad de primera, segunda y tercera estadio las larvas durante un intervalo de grabación de 20 min a 20 ° C. N = 32 para cada etapa larval. Figura 4. Histograma que muestra número medio de movimientos que se producen en cada minuto del intervalo de grabación 20 min. 32 larvas de tercer instar se ensayaron a 20 ° C. La línea roja representa el número de movimientos por minuto en promedio para todo el intervalo de 20 min. <img alt="Figura 5" src="/files/ftp_upload/52684/52684fig5.jpg" /> Figura 5. Diagrama que ilustra la Drosophila Activity Monitor puesta en marcha y su conectividad con la unidad de interfaz Psiu y una computadora de escritorio. El interior de la incubadora se representa, pero durante la grabación de la incubadora es que ser cerrado. <table border="0" cellpadding="0" cellspacing="0"><colgroup><col span="2" /></colgroup><tbody><tr><td> Descripción </td><td> Parámetro </td></tr><tr><td> Registros de datos cada vezuna larva atraviesa un rayo, y se registran los recuentos adicionales si la larva se mueve mientras dentro de un solo haz. </td><td> Condes </td></tr><tr><td> Registros de datos sólo cuando una mosca reposiciona entre vigas separadas, que no registra movimiento dentro de una viga. </td><td> Movimientos </td></tr><tr><td> Registra la posición de los animales en cada segundo durante un intervalo de grabación. Estos datos revelan la preferencia de posición como una función del tiempo pasado en cada sensor en el transcurso de un ensayo. </td><td> Morar </td></tr><tr><td> Esta configuración analiza la posición general del animal dentro del tubo, lo que indica que el sensor del animal está provocando durante el movimiento. </td><td> Posición </td></tr><tr><td> Este ajuste determina la frecuencia con la que los datos recogidos durante un plazo establecido se guardan en el ordenador de sobremesa. </td><td> Grabación a intervalos </td></tr></tbody></table> Tabla 1. Descripción de measuparámetros rement (Condes, Moves: Quédate y puestos). <img alt="Video 1" src="/files/ftp_upload/52684/52684vid1.jpg" /> Vídeo 1. DAM tubo de ensayo del sistema antes de la inserción en el dispositivo operativo. La humedad es proporcionada por la condensación del aliento. Este nivel es suficiente para mantener la locomoción de larvas durante todo el período de estudio, sin causar el animal para flotar o nadar. <a href="https://www.jove.com/files/ftp_upload/52684/McParlandlarvamovinginmoistassaytube.mov" target="_blank">Por favor, haga clic aquí para ver el vídeo.</a>

Watch this Scientific Journal Video about Measurement of Larval Activity in the Drosophila Activity Monitor at JoVE.com

Measurement of Larval Activity in the Drosophila Activity Monitor

This report describes a method for measuring Drosophila larval activity using the TriKinetics Drosophila Activity Monitor. The device employs infrared beams to detect movements of up to 16 individual animals. Data can be analyzed to represent motion parameters including rates and the positions of the animals within the assay chambers.

La medición de las larvas La actividad en el<em&gt; Drosophila</em&gt; Monitor de Actividad

Drosophila larvae are used in many behavioral studies, yet a simple device for measuring basic parameters of larval activity has not been available. This ...

measurement-of-larval-activity-in-the-drosophila-activity-monitor

Nanyang Technological University

Research

JoVE Journal

Biology

Measurement of Larval Activity in the Drosophila Activity Monitor

9.3K vistas.  University of New England. This report describes a method for measuring Drosophila larval activity using the TriKinetics Drosophila Activity Monitor. The device employs infrared beams to detect movements of up to 16 individual animals. Data can be analyzed to represent motion parameters including rates and the positions of the animals within the assay chambers.

Video: Measurement of Larval Activity in the Drosophila Activity Monitor

Dissection of Larval CNS in Drosophila Melanogaster

The central nervous system (CNS) of Drosophila larvae is complex and poorly understood.  One way to investigate the CNS is to use immunohistochemistry to examine the expression of various novel and marker proteins.  Staining of whole larvae is impractical because the tough cuticle prevents antibodies from penetrating inside the body cavity.  In order to stain these tissues it is necessary to dissect the animal prior to fixing and staining.  In this article we demonstrate how to dissect Drosophila larvae without damaging the CNS.  Begin by tearing the larva in half with a pair of fine forceps, and then turn the cuticle "inside-out" to expose the CNS.  If the dissection is performed carefully the CNS will remain attached to the cuticle.  We usually keep the CNS attached to the cuticle throughout the fixation and staining steps, and only completely remove the CNS from the cuticle just prior to mounting the samples on glass slides.  We also show some representative images of a larval CNS stained with Eve, a transcription factor expressed in a subset of neurons in the CNS.  The article concludes with a discussion of some of the practical uses of this technique and the potential difficulties that may arise.

In this article we demonstrate how to dissect the central nervous system from third instar Drosophila larvae.

La disección del sistema nervioso central de larvas de Drosophila melanogaster

The central nervous system (CNS) of Drosophila larvae is complex and poorly understood.  One way to investigate the CNS is to use immunohistochemistry to ...

Investigación

Biología

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 ...

Drosophila Larval NMJ Immunohistochemistry

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 31 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. Immunohistochemistry can be used to clearly image the components of the NMJ. In this article, we demonstrate how to use antibody staining to visualize the Drosophila larval NMJ.

Drosophila Larval NMJ Immunohistochemistry

This protocol demonstrates how to perform immunohistochemistry on dissected Drosophila larva.

Drosophila larval NMJ inmunohistoquímica

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 ...

Direct Detection of the Acetate-forming Activity  of the Enzyme Acetate Kinase

Acetate kinase, a member of the acetate and sugar kinase-Hsp70-actin (ASKHA) enzyme superfamily1-5, is responsible for the reversible phosphorylation of acetate to acetyl phosphate utilizing ATP as a substrate. Acetate kinases are ubiquitous in the Bacteria, found in one genus of Archaea, and are also present in microbes of the Eukarya6. The most well characterized acetate kinase is that from the methane-producing archaeon Methanosarcina thermophila7-14. An acetate kinase which can only utilize PPi but not ATP in the acetyl phosphate-forming direction has been isolated from Entamoeba histolytica, the causative agent of amoebic dysentery, and has thus far only been found in this genus15,16.
In the direction of acetyl phosphate formation, acetate kinase activity is typically measured using the hydroxamate assay, first described by Lipmann17-20, a coupled assay in which conversion of ATP to ADP is coupled to oxidation of NADH to NAD+ by the enzymes pyruvate kinase and lactate dehydrogenase21,22, or an assay measuring release of inorganic phosphate after reaction of the acetyl phosphate product with hydroxylamine23. Activity in the opposite, acetate-forming direction is measured by coupling ATP formation from ADP to the reduction of NADP+ to NADPH by the enzymes hexokinase and glucose 6-phosphate dehydrogenase24.
Here we describe a method for the detection of acetate kinase activity in the direction of acetate formation that does not require coupling enzymes, but is instead based on direct determination of acetyl phosphate consumption. After the enzymatic reaction, remaining acetyl phosphate is converted to a ferric hydroxamate complex that can be measured spectrophotometrically, as for the hydroxamate assay. Thus, unlike the standard coupled assay for this direction that is dependent on the production of ATP from ADP, this direct assay can be used for acetate kinases that produce ATP or PPi.

A method for the determination of acetate kinase activity is described. This assay utilizes a direct reaction for determining enzyme activity and kinetics of acetate kinase in the acetate-forming direction with different phosphoryl acceptors. Furthermore, this method can be utilized for assaying other acetyl phosphate or acetyl-CoA utilizing enzymes.

La detección directa de la actividad de acetato de formación de la enzima cinasa de acetato

Acetate kinase, a member of the acetate and sugar kinase-Hsp70-actin (ASKHA) enzyme superfamily1-5, is responsible for the reversible phosphorylation of ...

Assaying the Kinase Activity of LRRK2 in vitro

Leucine Rich Repeat Kinase 2 (LRRK2) is a 2527 amino acid member of the ROCO family of proteins, possessing a complex, multidomain structure including a GTPase domain (termed ROC, for Ras of Complex proteins) and a kinase domain1. The discovery in 2004 of mutations in LRRK2 that cause Parkinson's disease (PD) resulted in LRRK2 being the focus of a huge volume of research into its normal function and how the protein goes awry in the disease state2,3. Initial investigations into the function of LRRK2 focused on its enzymatic activities4-6. Although a clear picture has yet to emerge of a consistent alteration in these due to mutations, data from a number of groups has highlighted the importance of the kinase activity of LRRK2 in cell death linked to mutations7,8. Recent publications have reported inhibitors targeting the kinase activity of LRRK2, providing a key experimental tool9-11. In light of these data, it is likely that the enzymatic properties of LRRK2 afford us an important window into the biology of this protein, although whether they are potential drug targets for Parkinson's is open to debate.
A number of different approaches have been used to assay the kinase activity of LRRK2. Initially, assays were carried out using epitope tagged protein overexpressed in mammalian cell lines and immunoprecipitated, with the assays carried out using this protein immobilised on agarose beads4,5,7. Subsequently, purified recombinant fragments of LRRK2 in solution have also been used, for example a GST tagged fragment purified from insect cells containing residues 970 to 2527 of LRRK212. Recently, Dani&euml;ls et al. reported the isolation of full length LRRK2 in solution from human embryonic kidney cells, however this protein is not widely available13. In contrast, the GST fusion truncated form of LRRK2 is commercially available (from Invitrogen, see table 1 for details), and provides a convenient tool for demonstrating an assay for LRRK2 kinase activity. Several different outputs for LRRK2 kinase activity have been reported. Autophosphorylation of LRRK2 itself, phosphorylation of Myelin Basic Protein (MBP) as a generic kinase substrate and phosphorylation of an artificial substrate - dubbed LRRKtide, based upon phosphorylation of threonine 558 in Moesin - have all been used, as have a series of putative physiological substrates including &alpha;-synuclein, Moesin and 4-EBP14-17. The status of these proteins as substrates for LRRK2 remains unclear, and as such the protocol described below will focus on using MBP as a generic substrate, noting the utility of this system to assay LRRK2 kinase activity directed against a range of potential substrates.

Assaying the Kinase Activity of LRRK2 in vitro

Leucine Rich Repeat Kinase 2 is a large multidomain kinase, mutations in which are the most common genetic cause of Parkinson's disease. Analysis of the kinase activity of this protein has proven to be a crucial tool in understanding the biology and dysfunction of this protein. In this paper, in vitro assaying of the kinase activity of LRRK2 and a selection of its mutants is described, providing an experimental system to examine phosphorylation of putative substrates and potential dysfunction of LRRK2 in disease.

Ensayo de la actividad quinasa de LRRK2 In vitro</em

Leucine Rich Repeat Kinase 2 (LRRK2) is a 2527 amino acid member of the ROCO family of proteins, possessing a complex, multidomain structure including a ...

Measurement of Lifespan in Drosophila melanogaster

Aging is a phenomenon that results in steady physiological deterioration in nearly all organisms in which it has been examined, leading to reduced physical performance and increased risk of disease. Individual aging is manifest at the population level as an increase in age-dependent mortality, which is often measured in the laboratory by observing lifespan in large cohorts of age-matched individuals. Experiments that seek to quantify the extent to which genetic or environmental manipulations impact lifespan in simple model organisms have been remarkably successful for understanding the aspects of aging that are conserved across taxa and for inspiring new strategies for extending lifespan and preventing age-associated disease in mammals.
The vinegar fly, Drosophila melanogaster, is an attractive model organism for studying the mechanisms of aging due to its relatively short lifespan, convenient husbandry, and facile genetics. However, demographic measures of aging, including age-specific survival and mortality, are extraordinarily susceptible to even minor variations in experimental design and environment, and the maintenance of strict laboratory practices for the duration of aging experiments is required. These considerations, together with the need to practice careful control of genetic background, are essential for generating robust measurements. Indeed, there are many notable controversies surrounding inference from longevity experiments in yeast, worms, flies and mice that have been traced to environmental or genetic artifacts1-4. In this protocol, we describe a set of procedures that have been optimized over many years of measuring longevity in Drosophila using laboratory vials. We also describe the use of the dLife software, which was developed by our laboratory and is available for download (<a href="http://sitemaker.umich.edu/pletcherlab/software">http://sitemaker.umich.edu/pletcherlab/software</a>). dLife accelerates throughput and promotes good practices by incorporating optimal experimental design, simplifying fly handling and data collection, and standardizing data analysis. We will also discuss the many potential pitfalls in the design, collection, and interpretation of lifespan data, and we provide steps to avoid these dangers.

Measurement of Lifespan in Drosophila melanogaster

Drosophila melanogaster is a powerful model organism for exploring the molecular basis of longevity regulation. This protocol will discuss the steps involved in generating a reproducible, population-based measurement of longevity as well as potential pitfalls and how to avoid them.

Medición de la esperanza de vida en<em&gt; Drosophila melanogaster</em

Aging is a phenomenon that results in steady physiological deterioration in nearly all organisms in which it has been examined, leading to reduced ...

A Method of Permeabilization of Drosophila Embryos for Assays of Small Molecule Activity

The Drosophila embryo has long been a powerful laboratory model for elucidating molecular and genetic mechanisms that control development. The ease of genetic manipulations with this model has supplanted pharmacological approaches that are commonplace in other animal models and cell-based assays. Here we describe recent advances in a protocol that enables application of small molecules to the developing fruit fly embryo. The method details steps to overcome the impermeability of the eggshell while maintaining embryo viability. Eggshell permeabilization across a broad range of developmental stages is achieved by application of a previously described d-limonene embryo permeabilization solvent (EPS1) and by aging embryos at reduced temperature (18 &#176;C) prior to treatments. In addition, use of a far-red dye (CY5) as a permeabilization indicator is described, which is compatible with downstream applications involving standard red and green fluorescent dyes in live and fixed preparations. This protocol is applicable to studies using bioactive compounds to probe developmental mechanisms as well as for studies aimed at evaluating teratogenic or pharmacologic activity of uncharacterized small molecules.

A Method of Permeabilization of Drosophila Embryos for Assays of Small Molecule Activity

Introduction of small molecules to the developing Drosophila embryo offers great potential for characterizing biological activity of novel compounds, drugs, and toxins as well as for probing fundamental developmental pathways. Methods described herein outline steps that overcome natural barriers to this approach, expanding the utility of the Drosophila embryo model.

Un método de permeabilización de<em&gt; Drosophila</em&gt; Los embriones para ensayos de moléculas pequeñas Actividad

The Drosophila embryo has long been a powerful laboratory model for elucidating molecular and genetic mechanisms that control development. The ease of ...

Measurement of Metabolic Rate in Drosophila using Respirometry

Metabolic disorders are a frequent problem affecting human health. Therefore, understanding the mechanisms that regulate metabolism is a crucial scientific task. Many disease causing genes in humans have a fly homologue, making Drosophila a good model to study signaling pathways involved in the development of different disorders. Additionally, the tractability of Drosophila simplifies genetic screens to aid in identifying novel therapeutic targets that may regulate metabolism. In order to perform such a screen a simple and fast method to identify changes in the metabolic state of flies is necessary. In general, carbon dioxide production is a good indicator of substrate oxidation and energy expenditure providing information about metabolic state. In this protocol we introduce a simple method to measure CO2 output from flies. This technique can potentially aid in the identification of genetic perturbations affecting metabolic rate.

Measurement of Metabolic Rate in Drosophila using Respirometry

Metabolic disorders are among one of the most common diseases in humans. The genetically tractable model organism D. melanogaster can be used to identify novel genes that regulate metabolism. This paper describes a relatively simple method which allows studying the metabolic rate in flies by measuring their CO2 production.

La medición de la tasa metabólica en<em&gt; Drosophila</em&gt; Mediante respirometría

Metabolic disorders are a frequent problem affecting human health. Therefore, understanding the mechanisms that regulate metabolism is a crucial ...

Functional Reconstitution and Channel Activity Measurements of Purified Wildtype and Mutant CFTR Protein

The Cystic Fibrosis Transmembrane Conductance Regulator (CFTR) is a unique channel-forming member of the ATP Binding Cassette (ABC) superfamily of transporters. The phosphorylation and nucleotide dependent chloride channel activity of CFTR has been frequently studied in whole cell systems and as single channels in excised membrane patches. Many Cystic Fibrosis-causing mutations have been shown to alter this activity. While a small number of purification protocols have been published, a fast reconstitution method that retains channel activity and a suitable method for studying population channel activity in a purified system have been lacking. Here rapid methods are described for purification and functional reconstitution of the full-length CFTR protein into proteoliposomes of defined lipid composition that retains activity as a regulated halide channel. This reconstitution method together with a novel flux-based assay of channel activity is a suitable system for studying the population channel properties of wild type CFTR and the disease-causing mutants F508del- and G551D-CFTR. Specifically, the method has utility in studying the direct effects of phosphorylation, nucleotides and small molecules such as potentiators and inhibitors on CFTR channel activity. The methods are also amenable to the study of other membrane channels/transporters for anionic substrates.

Described here is a rapid and effective procedure for functional reconstitution of purified wild-type and mutant CFTR protein that preserves activity for this chloride channel, which is defective in Cystic Fibrosis. Iodide efflux from reconstituted proteoliposomes mediated by CFTR allows studies of channel activity and the effects of small molecules.