Bu çalışma, Ulusal Sağlık Enstitüsü, hibe NS27501 tarafından desteklenen DKOD. Bir HHMI Profesör Grant DKOD bu iş için ek destek.

I. Drosophila Embriyo Koleksiyonu <ol><li> Yumurta toplama plakaları hazırlayın <ol><li> 8 g agar ile kaynatın 200 ml dH 2 O </li><li> Soğuk - 50 ° C </li><li> 2 ml EtOH ve 2 ml asetik asit </li><li> 35 mm plastik petri kaplarına, tops dökün </li><li> Serin ve hava geçirmez bir kapta saklayın, 4 ° C </li><li> Yaklaşık 80 plakalar yapar </li></ol></li><li> Maya macun hazırlayın <ol><li> Hamur oluşturmak için Fleishmans aktif pişirme maya su içinde çözülür </li><li> Maya öldürmek için 20-30 saniye Mikro dalga fırın (Üzerine kaynar dikkat) </li><li> 4 ° C için 2 hafta, 10 cc şırınga (iğne) saklayın </li></ol></li><li> Sinekler: yumurta toplama için kullanılan yetişkin taze gıda erişim vardı koşuluyla, genellikle 3 ile 14 gün arasında ortaya çıkan sonra en verimli. Birçok mutant stokları yumurtlama ve en verimli hangi yaşta bir değişiklik indirdi oranı kendini gösterir doğurganlık azalmıştır. Genellikle iyi bir yumurtlama nüfus için, birkaç yüz yetişkin olun. </li><li> Prosedür: Bir yumurta toplama plakası yapıştırmak maya ince bir tabaka sürün. Bu yumurta döşenmesi için uygun bir substrat sağlar. Transferi yetişkin şişenin ağzına temiz bir yumurta toplama şişesi ve bant toplama plakası uçar. Nem oranı yükselir ve sinekler yapıştırın ve şişe tarafta takılıyorum 3-4 saatten daha uzun süre bu şişelerde sinekler terk etmeyin. </li></ol> II. Çamaşır suyu ile Embriyo Dechorionation <ol><li> Bir aspiratör bağlı bir filtre balonuna bağlı bir Buchner huni ayarlayın. Huni whatman # 1 kağıt parçası koyun. Emme çalışırken, kağıt steril distile su ile ıslatın. </li><li> Yıkama şişe su akışı ile filtre kağıdı üzerine toplama plakaları embriyolar durulayın. </li><li> Steril su çeşitli hacimlerde onları durulayın, aspiratör kapatmak ve daha sonra bir huni hacminin% 50 çamaşır suyu ekleyin. Yumurtalar 5-10 dakika bekletin. Chorions 1-2 dakika içinde çözünmüş, ama uzun süre daha fazla kirlenmesine neden olan maya yok edilecektir çamaşır embriyolar terk olacaktır. Çanak durulanır herhangi bir yetişkin veya larva dışarı seçin. </li><li> Steril distile su ile steril bir petri (doku kültürü DEĞİL) embriyolar durulayın. Önceden ıslatılmış edilmemiş ise embriyoların çoğu çanak alt sopa olacak. Bu yemeğin steril su ile birkaç kez durulayın. </li><li> Gastrula orta dönem embriyoların almak için iletilen ışık ile embriyolar inceleyin. </li></ol> III. Tek embriyo kültürlerin hazırlanması <ol><li> DDM1 (bölüm IV tarifleri görmek) gerçekleştirmek </li><li> Hemen önce kültür embriyo çanak kapalı su dökün. Embriyolar steril ortam ile kaplayın. </li><li> 3, 35 mm petri kaplarına ayarlayın. Her çanak 4 otoklavlanmış yuvarlak lamelleri koyun. Her lamel, 5 ul orta koydu. Bellco lamelleri düşük kurşun cam coverlips kullanın. Bellco Biyolojik Züccaciye 800-257-7043 Kedi # 1.943-00.012 </li><li> Bazı oldukça ince pipetler çekin. Kullandığımız pipetleri bir Narishige PP-83 çektirmesi çekti. Pipetlemeyin kesin boyutları çok önemli değildir ve genellikle onları bizim istediğimiz daha ince çekin ve onları boyutunu ölçmek için embriyo olarak aynı alanda ucu kesiyorum. Tek seferde tüm embriyoların emmek istiyor ve bu hücrelerin emmek için 5 dakika sürer ucu kadar küçük istemiyorum. Arasında bir yere yöneltin. Iletilen ışık ile embriyoların inceleyin ve embriyo içeriğini kaldırmak için pipetlemeyin bağlı bir ağız emme borusu kullanmayın. Lamel mümkün olduğunca yakın olarak hücrelerin nazikçe atarak hazırlanan lamel üzerine hücreler dağılırlar. Lamelleri yüksek bir güç düzeyinde incelemek istediğiniz ve hücrelerin daha aynı şekilde dağıtmak. </li><li> Hücreleri, 10 dakikadan daha uzun süre bekletin. Sel çanak medya ile ve inkübatör koymak,% 4-5 CO 2 ortamında tanımlanan orta kullanıyorsanız. Sıcaklık 22-24 arasında ° C Biz rutin olarak 23 ° C ve% 95 nem kullanın. Nem buharlaşmasını önlemek için istediğiniz gibi önemlidir. 23 ayarlanan sıcaklık kontrolü ile coldroom yerleştirilen standart bir memeli inkübatör ° C </li></ol> IV. Kültürler büyüyen DDM1 Tanımlı orta <ol><li> 100 ml Ham F12/DME Media (DMEM) (Irvine Scientific # 9052): DMEM Yapın <ol><li> 0.476 g HEPES (20mm) (Sigma # H-3375). Karıştırın. </li><li> 1.25 ml L-Glutamin 200 mM (# 9317 Irvine Scientific) ekleyin. Karıştırın. </li><li> Filtre 0.2 mikron asetat şırınga filtresi (2 filtrelere ihtiyaç) ile kaputu. </li><li> PH 6.64 ve OSM 288. </li><li> 15ml santrifüj tüplerine 10 ml hacimde olun. </li><li> 4 ° C en fazla 2 hafta saklayınız. Not: Daima yalnızca medya ve Takviyeler için ayrılmış kaplarda otoklavlanmış filtrelenmiş su kullanımı ve. Aşağıda listelenen ekle takviyeleri: pH elektrodu koymak ya da Asla Media.To diğer amaçlar için kullanılan bar karıştırın DDM1 olunkültür için DMEM hemen önce. </li></ol></li><li> DMEM eklemek için 10 ml: <ul><li> 100 ul Transferrin </li><li> 100 ul Putrescine </li><li> 100 ul Selenyum </li><li> 100 ul Progesteron </li><li> 50 ul İnsülin </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>

Midgastrula dönem embriyoların hazırlanan Drosophila kültürlerde nöronlar in vitro farklılaşma önce bölmek çoğu neuroblast öncüleri, ortaya çıkar. Bu sistem, böylece nöronal gelişiminin çok erken evrelerinde (Rohrbaugh ve ark, 2003) önemli genetik ve çevresel faktörlerin araştırılması için eşsiz bir fırsat sağlar. Biz, tanımlanmış basit bir ortamda yetişen nöronların elektriksel olarak uyarılabilen nöronların (Lee ve O Dowd, 1999 O Dowd, 1995) fonksiyonel sinaptik bağlantıları oluşturmak ayrım ol...

Bu medya yapılan kültürler, 22-24 ° C&#39;de% 5 CO2 inkübatör muhafaza edilmelidir Biz kuvöz soğuk bir odaya yerleştirilen bir standart memeli doku kültürü ve 23 ° C&#39;ye kadar ısıtılır Otoklavlanmış filtrelenmiş su ve yalnızca medya ve takviyeleri için ayrılmış kaplarda yapmak her zaman kullanılır. Bir pH metre koymak veya diğer amaçlar için kullanılan medya bar karıştırın.

preparation of neuronal cultures from midgastrula stage drosophila embryos

Bu video midgastrula evre Drosophila embriyolar primer nöronal kültürlerin yapmak için prosedür göstermektedir. Çamaşır suyu kullanarak embriyo ve kendi dechorionation toplama yöntemleri gösterilmektedir. Ağız emme borusu bağlı bir damlalıklı cam kullanarak, tüm hücreleri tek embriyolar kaldırılması göstermektedir. Kaplamasız bir cam lamel, orta (5 lt) küçük bir düşüş içine her embyro hücrelerini dağıtma yöntemi olduğunu göstermiştir. Kaplama 1 saat sonra mikroskop ile bir görünüm için tercih edilen bir hücre yoğunluğu göstermektedir. Tanımlanan orta büyüdüğü zaman hayatta hücrelerinin çoğu 12-24 saat nöritik süreçleri uzanan önce bir kez veya daha fazla kültür bölmek neuroblasts. Mikroskop aracılığıyla bir görünüm neurite akıbet seviyesini gösterir ve in vitro 2 gün sağlıklı bir kültür beklenen dallanma. Kültürleri, 22-24 ° C&#39;de% 5 CO 2 inkübatör tanımlanan orta tabanlı basit bir bikarbonat yetiştirilen Nöritik süreçleri kültürünün ilk haftasında ayrıntılı olarak devam etmek ve komşu hücrelerden genellikle fonksiyonel sinaptik bağlantıları formu neurites ile temas yaparken. Bu kültürlerin Nöronlar voltaj kapılı sodyum, kalsiyum ve potasyum kanalları ifade ve elektriksel olarak uyarılabilen. Bu kültür sistemi nöronal farklılaşma, heyecanlanma, ve sinaps oluşumu / fonksiyon düzenleyen moleküler genetik ve çevresel faktörlerin çalışmak için yararlıdır.

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

Bu video midgastrula evre Drosophila embriyolar primer nöronal kültürlerin hazırlanmasında gösteriyor. Canlı kültürlerin Görüntüleme kaplama 2 gün sonra bir bikarbonat tabanlı tanımlı bir ortamda büyüme ve farklı nöronlar sonra hücreler 1 saat gösteriyor. Nöronların elektriksel olarak uyarılabilen ve sinaptik bağlantıları formu.

Nöronal Kültürler Midgastrula Sahne Drosophila Embriyolar hazırlanması

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

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8.8K Görüntüleme.  University of California, Irvine (UCI). Bu video midgastrula evre Drosophila embriyolar primer nöronal kültürlerin hazırlanmasında gösteriyor. Canlı kültürlerin Görüntüleme kaplama 2 gün sonra bir bikarbonat tabanlı tanımlı bir ortamda büyüme ve farklı nöronlar sonra hücreler 1 saat gösteriyor. Nöronların elektriksel olarak uyarılabilen ve sinaptik bağlantıları formu.

Video: 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.

Geç Stage Drosophila pupa Brain İlköğretim Nöronal Kültürler

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

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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.

Erken Evre Tavuk Embriyolar Büyüme Faktörü-Kaplı Boncuk yerleştirme

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.

HH Sahne 10 Tavuk Embriyolar Ovo 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.

Büyüme Konileri Yüksek Çözünürlüklü Görüntüleme için Aplysia Nöronal Hücre Kültürleri

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.

Hazırlık Elektroporasyon murin Kemik İliği itibaren İlköğretim Hematopoetik Hücre Kültürleri

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.

Hazırlanması Drosophila</emAsma Bırak Protokolü kullanarak Canlı Görüntüleme> Embriyolar

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.

Hazırlanması Aplysia Duyusal-motor Nöronal Hücre Kültürleri

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.

Elektron Mikroskobu için embriyo Hazırlık Drosophila Embriyonik kalp tüpü

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.

In-vivo Drosophila Embriyolar Santrifüj

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.

Upright Imaging of Drosophila Embryos

Here we present a mounting protocol for stained Drosophila embryos in an upright position that allows imaging of cross-sections using Confocal microscopy.

VE Dik Görüntüleme Drosophila Embriyolar

Several well-known morphogenetic gradients and cellular movements occur along the dorsal/ventral axis of the Drosophila embryo. However, the current ...