这项工作是由美国国立卫生研究院授予NS27501 DKOD支持。这从霍华德休斯医学研究所教授格兰特DKOD工作的额外支持。

一，果蝇胚胎收集<ol><li>准备鸡蛋收集板<ol><li>煮沸200毫升与8克琼脂DH 2 O </li><li>冷却至50 ° C </li><li>加入2 ml乙醇和2毫升乙酸</li><li>倒入35 mm塑料培养皿中，上衣</li><li>酷存储在密封容器中，并在4 ° C </li><li>使大约80板</li></ol></li><li>准备酵母膏<ol><li>溶解于水Fleishmans积极烘烤酵母的形式粘贴</li><li> 20-30秒杀死酵母微波（小心沸腾了） </li><li>商店在10 CC（无针头注射器，在4 ° C的2个星期） </li></ol></li><li>苍蝇：用于鸡蛋收集的成年人通常是最有生产力的后3至14天之间出现，提供他们已经获得新鲜食品。许多突变的股票有生育能力，可以体现在降低了产蛋和改变他们是最有生产力的年龄，率下降。一般情况下，数百名成人为一个良好的产蛋人口。 </li><li>程序：一个鸡蛋收集板的粘贴，传播一层薄薄的酵母。这提供了一个有利的基板铺设鸡蛋。转移成蝇一个干净的鸡蛋收集瓶和磁带的收集板瓶口。不要离开苍蝇在这些瓶子超过3-4小时，湿度上升和苍蝇得到停留在粘贴和一瓶双方。 </li></ol>二。使用漂白剂的胚胎Dechorionation <ol><li>设置连接到一个连接到一个吸引器的滤瓶一个布氏漏斗。在漏斗放一块的Whatman＃1纸。吸运行，湿纸用无菌蒸馏水。 </li><li>到同一个流从洗瓶水冲洗滤纸收集板的胚胎。 </li><li>几卷的无菌水冲洗，关闭吸引器，然后添加50％的漂白粉漏斗量。让鸡蛋坐5-10分钟。 chorions会被溶解在1-2分钟，但你离开的时间越长在漂白剂的胚胎将被销毁的污染酵母。挑出任何成人或幼虫冲洗掉菜。 </li><li>的无菌培养皿中（而不是组织文化）用无菌蒸馏水冲洗胚胎。在胚胎中的许多人会坚持底部的菜，如果它没有被预湿。这个菜无菌水冲洗数次。 </li><li>与透射光下检查胚胎挑出中期原肠期胚胎。 </li></ol>三。制备单胚胎培养<ol><li>请DDM1（见第四节食谱） </li><li>倒掉水菜的胚胎前夕培养。封面用无菌媒体的胚胎。 </li><li> 3，35 mm培养皿。在4轮蒸压盖玻片，在每一道菜。在每个盖玻片，放5μL介质。使用Bellco盖玻片低铅玻璃coverlips。 Bellco生物玻璃器皿 800-257-7043 CAT＃1943-00012 </li><li>拉一些相当精细的吸管。我们使用的吸管被拉到一个Narishige PP - 83拉马。吸管的确切尺寸并不重要，我们通常拉他们比我们想的更细，他们打破了在相同的视野提示胚胎的大小来衡量。你不想吸了一口气所有的胚胎，你不想针尖那么小，它需要5分钟吸细胞。瞄准介于两者之间。与透射光下检查胚胎，使用口吸气管连接到吸管去除胚胎的内容。分散轻轻驱逐细胞尽可能靠近盖玻片准备盖玻片上的细胞。您可能要检查的盖玻片，在更高的功率，并进一步在以同样的方式驱散的细胞。 </li><li>让细胞不超过10分钟，坐。与媒体和洪水的菜放在培养箱中培养，4-5％的CO 2环境中，如果使用定义介质。温度介于22-24 ° C。我们经常使用的是23℃，湿度95％。湿度是重要的，只要你想，以避免蒸发。您可以使用放置在冷库温度控制标准的哺乳动物的孵化器设定至23 ° C。 </li></ol>四。 DDM1不断增长的文化定义介质<ol><li>设为DMEM培养液：100 MLS火腿的F12/DME媒体（DMEM）（＃9052）欧文分校的科学。 <ol><li>新增的0.476克羟乙基（20MM）（西格玛＃H - 3375）。混合。 </li><li>添加1.25毫升L -谷氨酰胺200毫米（尔湾科学＃9317）。混合。 </li><li>在0.2微米醋酸注射器过滤器（需要2个过滤器）过滤罩。 </li><li> pH值是6.64和OSM 288。 </li><li> 15ml离心管分装为10ml。 </li><li>储存于4 ° C下不超过2周。 注意：请务必使用蒸压过滤水，并在媒体和辅料只保留容器。永远不要把pH电极或搅拌Media.To其他用途使用的栏：下面列出的DDM1添加补充以DMEM培养液之前来培养。 </li></ol></li><li> 10毫升的DMEM中添加： <ul><li> 100μL转</li><li> 100μL腐胺</li><li> 100μL硒</li><li> 100μL孕酮</li><li> 50μL胰岛素</li></ul></li></ol>

<ol>
	<li>Rohrbough, J., O'Dowd, D. K., Baines, R. A., Broadie, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Cellular+bases+of+behavioral+plasticity:+Establishing+and+modifying+synaptic+circuits+in+the+Drosophila+Genetic+System.">Cellular bases of behavioral plasticity: Establishing and modifying synaptic circuits in the Drosophila Genetic System.</a> J. Neurobiol. 54, 254-271 (2003).</li><li>O'Dowd, D. K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Voltage-gated+currents+and+firing+properties+of+embryonic+Drosophila+neurons+grown+in+a+chemically+defined+medium.">Voltage-gated currents and firing properties of embryonic Drosophila neurons grown in a chemically defined medium.</a> J. Neurobiol. 27, 113-126 (1995).</li><li>Lee, D., O'Dowd, D. K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Fast+excitatory+synaptic+transmission+mediated+by+nAChR+in+cultured+Drosophila+neurons.">Fast excitatory synaptic transmission mediated by nAChR in cultured Drosophila neurons.</a> J. Neurosci. 19, 5311-5321 (1999).</li><li>Lee, D., O'Dowd, D. K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Cyclic-AMP-dependent+plasticity+at+excitatory+cholinergic+synapses+in+Drosophila+neurons:+Alterations+in+the+memory+mutant+dunce.">Cyclic-AMP-dependent plasticity at excitatory cholinergic synapses in Drosophila neurons: Alterations in the memory mutant dunce.</a> J. Neurosci. 20, 2104-2111 (2000).</li><li>Hodges, D. D., Lee, D., Boswell, K., Preston, C. F., Hall, L. M., O'Dowd, D. K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=tipE+regulates+sodium-dependent+repetitive+firing+in+Drosophila+neurons.">tipE regulates sodium-dependent repetitive firing in Drosophila neurons.</a> Mol. Cell Neurosci. 19, 402-416 (2002).</li><li>Lee, D., Su, H., Dowd, O., K, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=GABA+receptors+containing+Rdl+subunits+mediate+fast+inhibitory+synaptic+transmission+in+Drosophila+neurons.">GABA receptors containing Rdl subunits mediate fast inhibitory synaptic transmission in Drosophila neurons.</a> J. Neurosci. 23, 4625-4634 (2003).</li></ol>

在果蝇的文化准备midgastrula阶段的胚胎的神经元产生的，其中许多鸿沟之前，在体外分化成神经细胞前体。因此，该系统提供了一个独特的机会，在神经元发育的早期阶段（Rohrbaugh等，2003）中的重要探索遗传和环境因素。我们已经表明，生长在一个简单的定义介质的神经元分化成神经元电兴奋，也形成功能性突触连接（直径多德，1995年李和O多德，1999年）。使用分析突变体和/或药理操作，在这个模型系统可用于...

在这个媒体所作的文化，必须保持在5％CO2培养箱约22-24 ° C。我们使用一个标准的哺乳动物组织培养孵化器放置在寒冷的房间，并加热到23 ° C总是用灭菌过滤后的水，并在媒体和补充只保留容器。不要将pH计或搅拌媒体其他目的使用的栏。

preparation of neuronal cultures from midgastrula stage drosophila embryos

该视频演示了midgastrula阶段果蝇胚胎的主要神经文化的过程。收集胚胎和dechorionation使用漂白水的方法证明。我们说明了一嘴吸痰管使用玻璃吸管，从单一胚胎细胞清除。分散成小（5升）下降中等未涂层的玻璃盖玻片上的每一个embyro细胞的方法是证明。一个电镀后1小时，通过显微镜说明首选的细胞密度。大多数细胞的生存时，在定义中等增长是神经母细胞分裂前12-24小时延长神经炎进程的一个或多个次文化。通过显微镜说明突起生长的水平，预计在2天的体外分支在一个健康的文化。的文化是生长在一个简单的碳酸氢钠为主的定义介质在5％二氧化碳培养箱中培养，在22-24 ° C。神经炎进程继续阐述文化的第一个星期，当他们从邻近的细胞，他们往往形成功能性突触连接的突起联系。在这些文化中的神经元表达电压门控钠，钙，钾通道，电兴奋。这种文化系统是用于研究分子遗传和环境因素，调节神经细胞的分化，兴奋性突触的形成/功能。

Watch this Scientific Journal Video about Preparation of Neuronal Cultures from Midgastrula Stage Drosophila Embryos at JoVE.com

Preparation of Neuronal Cultures from Midgastrula Stage Drosophila Embryos

这个视频演示midgastrula阶段果蝇胚胎的主要神经文化的准备。生活文化的意见表明电镀和后2天在碳酸氢盐为基础的定义中等的增长有区别的神经元细胞1小时后。神经元电兴奋，并形成突触连接。

从Midgastrula舞台果蝇胚胎神经文化的制备

This video illustrates the procedure for making primary neuronal cultures from midgastrula stage Drosophila embryos. The methods for collecting embryos ...

preparation-neuronal-cultures-from-midgastrula-stage-drosophila

Research

JoVE Journal

Biology

8.8K 次观看.  University of California, Irvine (UCI). 这个视频演示midgastrula阶段果蝇胚胎的主要神经文化的准备。生活文化的意见表明电镀和后2天在碳酸氢盐为基础的定义中等的增长有区别的神经元细胞1小时后。神经元电兴奋，并形成突触连接。

视频: Preparation of Neuronal Cultures from Midgastrula Stage Drosophila Embryos

Primary Neuronal Cultures from the Brains of Late Stage Drosophila Pupae

In this video, we demonstrate the preparation of primary neuronal cultures from the brains of late stage Drosophila pupae. The procedure begins with the removal of brains from animals at 70-78 hrs after puparium formation. The isolated brains are shown after brief incubation in papain followed by several washes in serum-free growth medium. The process of mechanical dissociation of each brain in a 5 ul drop of media on a coverslip is illustrated. The axons and dendrites of the post-mitotic neurons are sheered off near the soma during dissociation but the neurons begin to regenerate processes within a few hours of plating. Images show live cultures at 2 days. Neurons continue to elaborate processes during the first week in culture. Specific neuronal populations can be identified in culture using GAL4 lines to drive tissue specific expression of fluorescent markers such as  GFP or RFP. Whole cell recordings have demonstrated the cultured neurons form functional, spontaneously active cholinergic and GABAergic synapses. A short video segment illustrates calcium dynamics in the cultured neurons using Fura-2 as a calcium indicator dye to monitor spontaneous calcium transients and nicotine evoked calcium responses in a dish of cultured neurons. These pupal brain cultures are a useful model system in which genetic and pharmacological tools can be used to identify intrinsic and extrinsic factors that influence formation and function of central synapses.

This video demonstrates the preparation of primary neuronal cultures from the brains of late stage Drosophila pupae. Views of live cultures show neurite outgrowth and imaging of calcium levels using Fura-2.

从晚期果蝇蛹的大脑原发性神经文化

In this video, we demonstrate the preparation of primary neuronal cultures from the brains of late stage Drosophila pupae. The procedure begins with the ...

科研

生物学

Placing Growth Factor-Coated Beads on Early Stage Chicken Embryos

The neural tube expresses many proteins in specific spatiotemporal patterns during development. These proteins have been shown to be critical for cell fate determination, cell migration, and formation of neural circuits. Neuronal induction and patterning involve bone morphogenetic protein (BMP), sonic hedgehog (SHH), fibroblast growth factor (FGF), among others. In particular, the expression pattern of Fgf8 is in close proximity to regions expressing BMP4 and SHH. This expression pattern is consistent with developmental interactions that facilitate patterning in the telencephalon.

Here we provide a visual demonstration of a method in which an in ovo preparation can be used to test the effects of Fgfs in the formation of the forebrain. Beads are coated with protein and placed in the developing neural tube to provide sustained exposure. Because the procedure uses small, carefully placed beads, it is minimally invasive and allows several beads to be placed within a single neural tube. Moreover, the method allows for continued development so that embryos can be analyzed at a more mature stage to detect changes in anatomy and in neural patterning. This simple but useful protocol allows for real time imaging. It provides a means to make spatially and temporally limited changes to endogenous protein levels.

A variety of growth factors and proteins interact to induce cells to take on different cell fates during development. Here we demonstrate the use of an in ovo preparation to address possible interactions between different proteins in development by placing beads on E2.5 chick embryos.

配售早期鸡胚生长因子包被的磁珠

The neural tube expresses many proteins in specific spatiotemporal patterns during development.   These proteins have been shown to be critical for cell ...

In Ovo Electroporations of HH Stage 10 Chicken Embryos

Large size and external development of the chicken embryo have long made it a valuable tool in the study of developmental biology.  With the advent of molecular biological techniques, the chick has become a useful system in which to study gene regulation and function.  By electroporating DNA or RNA constructs into the developing chicken embryo, genes can be expressed or knocked down in order to analyze in vivo gene function.  Similarly, reporter constructs can be used for fate mapping or to examine putative gene regulatory elements.  Compared to similar experiments in mouse, chick electroporation has the advantages of being quick, easy and inexpensive.  This video demonstrates first how to make a window in the eggshell to manipulate the embryo.  Next, the embryo is visualized with a dilute solution of India ink injected below the embryo.  A glass needle and pipette are used to inject DNA and Fast Green dye into the developing neural tube, then platinum electrodes are placed parallel to the embryo and short electrical pulses are administered with a pulse generator.  Finally, the egg is sealed with tape and placed back into an incubator for further development.  Additionally, the video shows proper egg storage and handling and discusses possible causes of embryo loss following electroporation.

Chick in ovo electroporation is a technique which allows genetic manipulation of the avian embryo. Common applications of this technique include functional analysis of genes and putative enhancer elements. This video demonstrates neural tube electroporation in HH 10 chick embryos. Injection technique and proper egg handling are discussed.

在OVO的HH阶段10个鸡胚Electroporations

Large size and external development of the chicken embryo have long made it a valuable tool in the study of developmental biology.  With the advent of ...

Neuronal Cell Cultures from Aplysia for High-Resolution Imaging of Growth Cones

Neuronal growth cones are the highly motile structures at the tip of axons that can detect guidance cues in the environment and transduce this information into directional movement towards the appropriate target cell. To fully understand how guidance information is transmitted from the cell surface to the underlying dynamic cytoskeletal networks, one needs a model system suitable for live cell imaging of protein dynamics at high temporal and spatial resolution. Typical vertebrate growth cones are too small to quantitatively analyze F-actin and microtubule dynamics. Neurons from the sea hare Aplysia californica are 5-10 times larger than vertebrate neurons, can easily be kept at room temperature and are very robust cells for micromanipulation and biophysical measurements. Their growth cones have very defined cytoplasmic regions and a well-described cytoskeletal system. The neuronal cell bodies can be microinjected with a variety of probes for studying growth cone motility and guidance. In the present protocol we demonstrate a procedure for dissection of the abdominal ganglion, culture of bag cell neurons and setting up an imaging chamber for live cell imaging of growth cones.

Aplysia californica neurons develop large growth cones in culture that are excellent for high-resolution imaging of growth cone motility and guidance. Here, we present a protocol for dissection and plating of Aplysia bag cell neurons as well as for setting up a chamber for live cell imaging.

从海兔的神经细胞培养的高分辨率成像生长锥

Neuronal growth cones are the highly motile structures at the tip of axons that can detect guidance cues in the environment and transduce this information ...

The Preparation of Primary Hematopoietic Cell Cultures From Murine Bone Marrow for Electroporation

It is becoming increasingly apparent that electroporation is the most effective way to introduce plasmid DNA or siRNA into primary cells. The Gene Pulser MXcell  electroporation system and Gene Pulser  electroporation buffer were specifically developed to transfect nucleic acids into mammalian cells and difficult-to-transfect cells, such as primary and stem cells.This video demonstrates how to establish primary hematopoietic cell cultures from murine bone marrow, and then prepare them for electroporation in the MXcell system. We begin by isolating femur and tibia. Bone marrow from both femur and tibia are then harvested and cultures are established. Cultured bone marrow cells are then transfected and analyzed.

This procedure describes how to establish primary hematopoietic cell cultures from murine bone marrow and is followed by transfection using the Gene Pulser MXCell electroporation system.

主电穿孔的小鼠骨髓造血细胞培养制备

It is becoming increasingly apparent that electroporation is the most effective way to introduce plasmid DNA or siRNA into primary cells. The Gene Pulser ...

The Preparation of Drosophila Embryos for Live-Imaging Using the Hanging Drop Protocol

Green fluorescent protein (GFP)-based timelapse live-imaging is a powerful technique for studying the genetic regulation of dynamic processes such as tissue morphogenesis, cell-cell adhesion, or cell death. Drosophila embryos expressing GFP are readily imaged using either stereoscopic or confocal microscopy. A goal of any live-imaging protocol is to minimize detrimental effects such as dehydration and hypoxia. Previous protocols for preparing Drosophila embryos for live-imaging analysis have involved placing dechorionated embryos in halocarbon oil and sandwiching them between a halocarbon gas-permeable membrane and a coverslip1-3. The introduction of compression through mounting embryos in this manner represents an undesirable complication for any biomechanical-based analysis of morphogenesis. Our method, which we call the hanging drop protocol, results in excellent viability of embryos during live imaging and does not require that embryos be compressed. Briefly, the hanging drop protocol involves the placement of embryos in a drop of halocarbon oil that is suspended from a coverslip, which is, in turn, fixed in position over a humid chamber. In addition to providing gas exchange and preventing dehydration, this arrangement takes advantage of the buoyancy of embryos in halocarbon oil to prevent them from drifting out of position during timelapse acquisition. This video describes in detail how to collect and prepare Drosophila embryos for live imaging using the hanging drop protocol. This protocol is suitable for imaging dechorionated embryos using stereomicroscopy or any upright compound fluorescence microscope.

The Preparation of Drosophila Embryos for Live-Imaging Using the Hanging Drop Protocol

A simple, inexpensive, and effective method of preparing Drosophila embryos for live-imaging analysis is presented. Our protocol provides humidity and gas exchange and does not compress the Drosophila embryo. This method is suitable for GFP-based live imaging of Drosophila embryos using a stereomicroscope or upright compound microscope.

编制果蝇实时成像的胚胎使用悬滴协议

Green fluorescent protein (GFP)-based timelapse live-imaging is a powerful technique for studying the genetic regulation of dynamic processes such as ...

Preparation of Aplysia Sensory-motor Neuronal Cell Cultures

The nervous system of the marine mollusk Aplysia californica is relatively simple, consisting of approximately 20,000 neurons. The neurons are large (up to 1 mm in diameter) and identifiable, with distinct sizes, shapes, positions and pigmentations, and the cell bodies are externally exposed in five paired ganglia distributed throughout the body of the animal. These properties have allowed investigators to delineate the circuitry underlying specific behaviors in the animal1. The monosynaptic connection between sensory and motor neurons is a central component of the gill-withdrawal reflex in the animal, a simple defensive reflex in which the animal withdraws its gill in response to tactile stimulation of the siphon. This reflex undergoes forms of non-associative and associative learning, including sensitization, habituation and classical conditioning. Of particular benefit to the study of synaptic plasticity, the sensory-motor synapse can be reconstituted in culture, where well-characterized stimuli elicit forms of plasticity that have direct correlates in the behavior of the animal2,3. Specifically, application of serotonin produces a synaptic strengthening that, depending on the application protocol, lasts for minutes (short-term facilitation), hours (intermediate-term facilitation) or days (long-term facilitation). In contrast, application of the peptide transmitter FMRFamide produces a synaptic weakening or depression that, depending on the application protocol, can last from minutes to days (long-term depression). The large size of the neurons allows for repeated sharp electrode recording of synaptic strength over periods of days together with microinjection of expression vectors, siRNAs and other compounds to target specific signaling cascades and molecules and thereby identify the molecular and cell biological steps that underlie the changes in synaptic efficacy.
An additional advantage of the Aplysia culture system comes from the fact that the neurons demonstrate synapse-specificity in culture4,5. Thus, sensory neurons do not form synapses with themselves (autapses) or with other sensory neurons, nor do they form synapses with non-target identified motor neurons in culture. The varicosities, sites of synaptic contact between sensory and motor neurons, are large enough (2-7 microns in diameter) to allow synapse formation (as well as changes in synaptic morphology) with target motor neurons to be studied at the light microscopic level.
In this video, we demonstrate each step of preparing sensory-motor neuron cultures, including anesthetizing adult and juvenile Aplysia, dissecting their ganglia, protease digestion of the ganglia, removal of the connective tissue by microdissection, identification of both sensory and motor neurons and removal of each cell type by microdissection, plating of the motor neuron, addition of the sensory neuron and manipulation of the sensory neurite to form contact with the cultured motor neuron.

Preparation of Aplysia Sensory-motor Neuronal Cell Cultures

Primary cultures of Aplysia sensory-motor neurons provide a model preparation for studying synapse formation and synaptic plasticity in vitro. This video demonstrates the identification and microdissection of sensory and motor neurons from Aplysia ganglia as well as the methods for establishing and maintaining sensory-motor neurons in culture.

制备海兔感觉运动神经元细胞培养

The nervous system of the marine mollusk Aplysia californica is relatively simple, consisting of approximately 20,000 neurons.  The neurons are large (up ...

Preparation of embryos for Electron Microscopy of the Drosophila embryonic heart tube

The morphogenesis of the Drosophila embryonic heart tube has emerged as a valuable model system for studying cell migration, cell-cell adhesion and cell shape changes during embryonic development. One of the challenges faced in studying this structure is that the lumen of the heart tube, as well as the membrane features that are crucial to heart tube formation, are difficult to visualize in whole mount embryos, due to the small size of the heart tube and intra-lumenal space relative to the embryo. The use of transmission electron microscopy allows for higher magnification of these structures and gives the advantage of examining the embryos in cross section, which easily reveals the size and shape of the lumen. In this video, we detail the process for reliable fixation, embedding, and sectioning of late stage Drosophila embryos in order to visualize the heart tube lumen as well as important cellular structures including cell-cell junctions and the basement membrane.

Preparation of embryos for Electron Microscopy of the Drosophila embryonic heart tube

We describe a process for fixation, embedding, sectioning, and imaging of late stage Drosophila embryos for Trasmission Electron Microscopy of the embryonic heart tube. This technique allows for the visualization of the heart tube lumen as well as the basement membrane, which lines the lumen of the heart.

电子显微镜对胚胎的制备果蝇胚胎心管

The morphogenesis of the Drosophila  embryonic heart tube has emerged as a valuable model system for studying cell migration, cell-cell adhesion and cell ...

In-vivo Centrifugation of Drosophila Embryos

A major strategy for purifying and isolating different types of intracellular organelles is to separate them from each other based on differences in buoyant density. However, when cells are disrupted prior to centrifugation, proteins and organelles in this non-native environment often inappropriately stick to each other. Here we describe a method to separate organelles by density in intact, living Drosophila embryos. Early embryos before cellularization are harvested from population cages, and their outer egg shells are removed by treatment with 50% bleach. Embryos are then transferred to a small agar plate and inserted, posterior end first, into small vertical holes in the agar. The plates containing embedded embryos are centrifuged for 30 min at 3000g. The agar supports the embryos and keeps them in a defined orientation. Afterwards, the embryos are dug out of the agar with a blunt needle. Centrifugation separates major organelles into distinct layers, a stratification easily visible by bright-field microscopy. A number of fluorescent markers are available to confirm successful stratification in living embryos. Proteins associated with certain organelles will be enriched in a particular layer, demonstrating colocalization. Individual layers can be recovered for biochemical analysis or transplantation into donor eggs. This technique is applicable for organelle separation in other large cells, including the eggs and oocytes of diverse species.

In-vivo Centrifugation of Drosophila Embryos

We describe a method to separate organelles by density in living Drosophila embryos. Embryos are embedded in agar and centrifuged. This technique yields reproducible separation of major organelles along the anterior-posterior embryo axis. This method facilitates colocalization experiments and yields organelle fractions for biochemical analysis and transplantation experiments.

果蝇胚胎的体内离心

A major strategy for purifying and isolating different types of intracellular organelles is to separate them from each other based on differences in ...

Upright Imaging of Drosophila Embryos

Several well-known morphogenetic gradients and cellular movements occur along the dorsal/ventral axis of the Drosophila embryo. However, the current techniques used to view such processes are somewhat limited. The following protocol describes a new technique for mounting fixed and labeled Drosophila embryos for coronal viewing with confocal imaging. This method consists of embedding embryos between two layers of glycerin jelly mounting media, and imaging jelly strips positioned upright. The first step for sandwiching the embryos is to make a thin bedding of glycerin jelly on a slide. Next, embryos are carefully aligned on this surface and covered with a second layer of jelly. After the second layer is solidified, strips of jelly are cut and flipped upright for imaging. Alternatives are described for visualizing the embryos depending upon the type of microscope stand to be used. Since all cells along the dorsal-ventral axis are imaged within a single confocal Z-plane, our method allows precise measurement and comparison of fluorescent signals without photobleaching or light scattering common to 3D reconstructions of longitudinally mounted embryos.