Yazarlar Sharmin Hossain SCE micromicropipette ipuçları elektron mikroskobu görüntüleri olgunlaşmamış bir nöron ve Derek Dunfield time-lapse yakalama büyüme için teşekkür ederiz.

Ekipman set-up: <ol><li> Bu teknik için gerekli elektrik ekipmanları, bir uyarıcıdır bir osiloskop ve gümüş tel mikropipet eklenecek ile donatılmış bir mikropipet sahibi. Biz genellikle bir Axon aletleri Axoporator 800A cihazın kullanımı, ancak bu Çim aletleri gibi diğer yaygın uyarıcıları SD9 uyarıcıları tek hücreli elektroporasyon için de uygundur. Cihazda dahili bir iletken solüsyon içeren cam mikropipet içine yerleştirilen gümüş tel elektrot ile arayüzleri headstage, bağlanır. Stimülatörü diğer kurşun tetra dış yerden giriş aldığı osiloskop girişi, bağlı. Tetra dış zemin elektroporasyon sırasında tetra electrotonic temas halinde kalan bir gümüş tel. Mikropipet larva ile temas konulduğunda devreyi tamamlamak. </li><li> Bu manevranın oda verir ve yaklaşık 30-45 derecelik bir açıyla mikropipet getirilerek sağlar yılından bu yana tek bir hücre elektroporasyon, iyi bir çalışma mesafesi (en az 5 cm) olan bir mikroskop gerektirir. </li></ol> Mikropipetler Fabrikasyon: Uygun mikropipetler hazırlanması, bu protokol için önemli bir adımdır. Buradaki zorluk, dar bir ucu (çapı 1 mikrona kadar) daha az doku delinmesiyle zaman kolayca kırmayacak bir dengeleme yatıyor. Ayrıca, 10 dereceden daha fazla bir konik açısı ile ipuçları çok tercih edildiğini bulduk. <ol><li> 1 mikrona kadar daha az bir ucu çapı ve 10 dereceden daha fazla bir ucu konik açısı ile çekilmiş bir cam mikropipet hazırlayın. <ol><li> Dış çapı 1.5mm ve 0.75mm iç çapı ile bir iç filament borosilikat cam ve bu amaç için uygundur. <ol><li> Nispeten daha kalın bir cam ucu katılık derecesi sağlar. </li><li> Iç filament mikropipet ucuna doğru geri-sıvı dolu çizim önemlidir. </li></ol></li></ol></li><li> Uygun ipuçları Fabrikasyon sıklıkla gözlenen sonuçların dayalı bazı değişiklikler gerekecektir. Farklı dokular, biraz daha farklı bir şekil veya bahşiş çapı bir ipucu isteyebilir. </li></ol> Tek hücreli elektroporasyon protokolü: Yeni kullanıcılar için, genetik olarak kodlanmış floresan proteinleri aksine, onlar hemen Epifloresans altında görülebilir, çünkü floresan dekstran boyalar ile başlamak tavsiye edilir. Floresan boyaların kullanımı kullanıcının doğrudan doku içinde mikropipet ucunun yerini görmek için sağlar ve üzerine elektroporasyon ekipman düzgün mikropipet ucu uygun olup olmadığını kurmak ve olup olmadığını anında geri bildirim verir. <ol><li> Mikropipet bir yükleme şırınga kullanarak veya arka doldurarak electroporated bileşik solüsyonu ile doldurun. <ol><li> Eğer plazmid DNA&#39;sı kullanarak, suda hazırlanan örnekleri endotoksin ücretsiz olduğunu sağlamak ve 1-2μg/ml arasında bir konsantrasyon. </li><li> Floresan dekstran boyaların konsantrasyonu ampirik olarak tespit edilmelidir. Biz sık sık su yaklaşık 300μM sulandırılmış floresan boya kullanın. </li><li> Tipik olarak, 0.5-1μl hacimleri yeterlidir. </li><li> Yüklemeden önce, kısaca tıkanmaya yol açabilir mikropipet, içine çekilir partikül enkaz miktarını azaltmak için yüksek hızda çözümler santrifüj. </li><li> Ucu içinde hava kabarcıkları genellikle akım etkileyebilir ve şiddetle headstage, montaj öncesinde mikropipet Flicking yerinden olmalıdır. </li></ol></li><li> Tutucunun içine mikropipet yerleştirin veya headstage, 3-eksen mikromanipülatör üzerine monte edilmiş. Mikropipet o gümüş tel elektrot yerleştirilir ve iç çözümü ile electrotonic temas içinde olduğunu emin olun. </li><li> Larva yetiştirme ortamı (Steinberg solüsyonu, pH 7.4) hazırlanan% 0,02 MS-222 (3-aminobenzoik asit etil ester) batırılarak tetarlar anestezisi. <ol><li> Biz normalde deneylerde evre 44-48 albino Xenopus laevis tetarlar kullanın. </li><li> Tetarlar yaklaşık 5 dakika sonra genellikle tamamen anestezi. </li><li> Çeşitli tetarlar bekleme süresini azaltmak için aynı anda narkoz olabilir, ancak 1 saat dışındaki süreler için MS-222 maruz kalmaktan kaçının. </li></ol></li><li> Plastik bir transfer mikropipet kullanarak elektroporasyon odasına tek bir anestezi larva transferi. <ol><li> Elektroporasyon odası, küçük bir Sylgard ® silikon blok tetra-şekilli bir kavite, oyma ve gümüş bir topraklama kablosu takmadan odasında larva ile electrotonic temas halinde olacağı gibi boşluğuna kolayca ev yapılabilir. </li></ol></li><li> Kullanılarak pozisyon larva dorsal tarafına fırça temizleyin. </li><li> Mikropipet, cilt ile temas halinde doğrudan ilgi bölgeye bitişik olduğu kadar düşürün. <ol><li> Yoğun dolu hücre gövdeleri bölgeleri hedeflemek, başarılı elektroporasyon şansını büyük ölçüde artıracaktır.Biz genellikle, tetra optik tectum hedef. </li><li> 30 ila 45 derecelik bir açıyla mikropipet getirin. Dik açıları genellikle bir görüşü engelleyen ise, sığ yörüngeleri, cilt ponksiyon daha zor hale getirir. </li></ol></li><li> Devamı mikropipet düşürücü cilt başlangıçta Köşelerini ve altta yatan doku içine geçmesine olacak. <ol><li> Yüzeysel hücreleri in vivo görüntüleme için tercih edilir ve mikropipet ucu cilt dimpling üzerine yavaş yavaş indirilir sağlamak hedeflenmiş olabilir. </li></ol></li><li> Bir kez dokusu içinde yer mikropipet direnci sürekli izlemeniz gerekir. Eğer bir Axoporator 800A (Axon Instruments), yaklaşık 10-40MΩ dirençler kullanarak en uygun olan. Direnç ucu çapı tek hücreli elektroporasyon için uygun olup olmadığını iyi bir gösterge. <ol><li> Yüksek mikropipet dirençleri (&gt; 100MΩ), çok dar ipuçları ile tıkanmış ip uçlarına ya da mikropipetler göstergesidir. </li><li> Düşük mikropipet dirençleri (10M), genellikle, bir kırık ucu bir sonucu çok büyük bir ucu çapı göstergesidir. </li><li> Doğrudan direncini ölçmek sağlamaz stimülatörü kullanıyorsanız, mikropipet direnç osiloskop (aşağıda) ele tarafından ölçülen gerilim darbeleri genliği gözlemleyerek dolaylı ölçülebilir. </li></ol></li><li> Gerilim tren uygulayın. <ol><li> Plazmid DNA için, darbe, darbe tren süresi 500ms 300Hz&#39;de teslim süresi 1ms negatif kare dalga bakliyat, oluşan en etkili olduğu tespit eğitir. <ol><li> Darbe gerilimi osiloskop ölçülen genlik bakliyat 0.75 ve 1.5μA arasında olduğunu ampirik gibi belirlenir. </li></ol></li><li> Floresan dekstran boyalar için, pozitif kare dalga darbeleri 300μs süresi 10ms darbe tren süresi ile 300Hz frekans teslim edilir. <ol><li> DNA protokol ile, darbe gerilimi osiloskop ölçülen genlik bakliyat 0.75 ve 1.5μA arasında olduğunu ampirik gibi belirlenir. </li><li> Epifloresans altında elektroporasyon sonuçlarını gözlemleyerek dayalı uyaran parametrelerine ek ayarlamalar yapılabilir. <ol><li> Electroporated hücreler loş görünür hücreleri parlak görünene kadar, darbe parametreleri giderek artmış olmalıdır. </li><li> Öte yandan hücre kümeleri etiketli, tek hücre etiketli kadar, darbe parametrelerin azaltılması olmalıdır. </li></ol></li></ol></li></ol></li><li> Mikropipet geri çekin, doku içinde farklı bir site tekrar takın, ve gerilim tren uygulayın. <ol><li> Verimi artırmak için, biz genellikle o etiketli hücrelerin üst üste binmemesi sağlamak için yeterli boşluk ile larva optik tectum her yarımkürede birden fazla sitede electroporate. </li></ol></li><li> Steinberg yetiştirme çözümü ile bir kap içine electroporated larva transferi. <ol><li> Tetarlar anestezi birkaç dakika içinde hızla iyileşir. </li></ol></li><li> Aynı mikropipet sayısız iribaşların kullanılabilir. Osiloskop gözlenen bakliyat genliği sürekli gözlemlemek önemlidir. <ol><li> Darbe genlik darbe yoğunluğu önemli ölçüde artan sonra düşük kalırsa, bu durum, bir oturuşta birçok tetarlar electroporating sık görülen tıkanmış olan ucu, bir sonucudur. <ol><li> Küçük bir ipucu yapışmasına neden çıkarmak için kullanılan bir yöntem, doku içine mikropipet yerleştirdikten sonra tek bir pozitif darbe uygulamaktır. </li><li> Yapışmasına neden yerinden ya da sık sık kendini yinelemektedir tıkanma değil, mikropipet değiştirin. </li></ol></li><li> Darbe genlik nabız parametrelerini önemli ölçüde azalan sonra çok büyük kalırsa, bu, ucu kırık olduğunu ve değiştirilmesi gerekir bir işaretidir. </li></ol></li></ol> Başarıyla electroporated hücreler için Gösterimi: <ol><li> Elektroporasyon sonra, tetarlar Epifloresans dik bir mikroskop kullanılarak etiketli hücreler için taranmaktadır. </li><li> Floresan boyaların durumda, en az 30 dakika sonrası elektroporasyon tetarlar sonra gösterilebilir. <ol><li> Biz daha uzun aralıklarla düşük eşiğe düzeyleri ile ilişkili olduğunu, ancak bulduk. </li></ol></li><li> Genetik olarak kodlanmış floresan proteinleri için, tarama genellikle en az 12 saat sonrası elektroporasyon yapılır. <ol><li> Floresan proteinlerle ifade hücreler zamanla parlak almaya devam edecektir, bu yüzden loş hücreleri 12-24 saat ek bir aradan sonra yeniden gösterildi olabilir. </li></ol></li><li> Sylgard ® odasında yerleştirilen, yukarıda açıklanan ve dakika muamele tetarlar anestezi. Bireysel tetarlar sonra Epifloresans altında incelenir. <ol><li> Epifloresans ışığa aşırı derecede maruz etiketli hücre öldürebilir fototoksisite neden olacağını unutmayın. Bu nedenle, floresan ışık hücrelerinin maruz kaldığı süreyi en aza indirir. </li></ol></li><li> Steinberg yetiştirme çözümü ile konteyner tetarlar dönün. </li></ol>

<ol>
	<li>Bestman, J. E., Ewald, R. C., Chiu, S. L., Cline, H. T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=In+vivo+single-cell+electroporation+for+transfer+of+DNA+and+macromolecules.">In vivo single-cell electroporation for transfer of DNA and macromolecules.</a> Nature Protocols. 1, 1267-1272 (2006).</li><li>Dunfield, D., Haas, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Single+cell+electroporation.">Single cell electroporation.</a> Encyclopedia of Neuroscience (4th Ed.). , .</li><li>Haas, K., Jensen, K., Sin, W. C., Foa, L., Cline, H. T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Targeted+electroporation+in+Xenopus+tadpoles+in+vivo--from+single+cells+to+the+entire+brain.">Targeted electroporation in Xenopus tadpoles in vivo--from single cells to the entire brain.</a> Differentiation. 70, 148-154 (2002).</li><li>Haas, K., Sin, W. C., Javaherian, A., Cline, H. T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Single-cell+electroporation+for+gene+transfer+in+vivo.">Single-cell electroporation for gene transfer in vivo.</a> Neuron. 29, 583-591 (2001).</li></ol>

Tek hücreli elektroporasyon (SCE), gen fonksiyonu belirleyen ve hedeflenen genetik manipülasyon yapmak için güçlü bir araçtır. Albino larva şeffaflık ve beyin erişilebilirlik Bu model sistem canlı bir organizma içinde nöronal büyüme ve hücre içi olayları görselleştirmek için ideal olun. SCE, tek bir nöronun büyüme görselleştirme izin verir, ve aksi halde değiştirilmemiş beynin içinde hücre özerk manipülasyonlar gerçekleştirebilirsiniz. Bu video makale Xenopus laevis tetarlar tek hücreli elektroporasyon i...

single cell electroporation in vivo within the intact developing brain

Tek hücreli elektroporasyon (SCE), in vivo hazırlıkları da dahil olmak üzere sağlam doku içindeki tek tek hücrelerin içine DNA veya diğer makromoleküller teslim sağlayan özel bir tekniktir. Bu tekniğin en belirgin avantajı, çevresindeki doku değişmeden bırakarak bu deneysel manipülasyonlar ve böylece küresel tedaviler sonucunda hücre özerk etkileri ayırt bireysel hücreleri üzerinde olabilir. Ileri in vivo görüntüleme teknikleri ile kombine edildiğinde, floresan belirteçlerin SCE hücresel morfoloji, hücre büyümesi ve hücre içi olayları saniye gün değişen zaman çizelgesi üzerinde doğrudan görselleştirme izin verir. Bu tekniği, in vivo ve ex vivo hazırlıkları içinde çeşitli olsa da, biz Xenopus laevis tetarlar kullanmak için bu tekniği optimize var. Bu video makalede, detaylı albino Xenopus larva bozulmamış beyin içinde nöronlar bir floresan boya veya plazmid DNA SCE prosedürü. Ayrıca verim optimize yöntemleri tartışmak ve canlı SCE tarafından floresan etiketli nöronlar iki foton floresan görüntüleme örnekler göstereceğiz.

Watch this Scientific Journal Video about Single Cell Electroporation in vivo within the Intact Developing Brain at JoVE.com

Single Cell Electroporation in vivo within the Intact Developing Brain

Tek hücreli elektroporasyon (SCE), in vivo hazırlıkları da dahil olmak üzere sağlam doku içindeki tek tek hücrelerin içine DNA veya diğer makromoleküller teslim sağlayan özel bir tekniktir. Xenopus laevis larva bozulmamış beyin içinde nöronların bir floresan boya veya plazmid DNA SCE için burada ayrıntılarıyla prosedür.

Tek Hücre Elektroporasyon bozulmamış Gelişmekte olan beyin içindeki in vivo

Single-cell electroporation (SCE) is a specialized technique allowing the delivery of DNA or other macromolecules into individual cells within intact ...

single-cell-electroporation-in-vivo-within-the-intact-developing-brain

Research

JoVE Journal

Biology

13.2K Görüntüleme.  University of British Columbia - UBC. Tek hücreli elektroporasyon (SCE), in vivo hazırlıkları da dahil olmak üzere sağlam doku içindeki tek tek hücrelerin içine DNA veya diğer makromoleküller teslim sağlayan özel bir tekniktir. Xenopus laevis larva bozulmamış beyin içinde nöronların bir floresan boya veya plazmid DNA SCE için burada ayrıntılarıyla prosedür.

Video: Single Cell Electroporation in vivo within the Intact Developing Brain

Electroporation of Mycobacteria

High efficiency transformation is a major limitation in the study of mycobacteria. The genus Mycobacterium can be difficult to transform; this is mainly caused by the thick and waxy cell wall, but is compounded by the fact that most molecular techniques have been developed for distantly-related species such as Escherichia coli and Bacillus subtilis. In spite of these obstacles, mycobacterial plasmids have been identified and DNA transformation of many mycobacterial species have now been described. The most successful method for introducing DNA into mycobacteria is electroporation. Many parameters contribute to successful transformation; these include the species/strain, the nature of the transforming DNA, the selectable marker used, the growth medium, and the  conditions for the electroporation pulse. Optimized methods for the transformation of both slow- and fast-grower are detailed here. Transformation efficiencies for different mycobacterial species and with various selectable markers are reported.

Mycobacterial pathogenic strategies remain poorly understood. The slow growth rate of most species, the impenetrable nature of the cell-wall, and the hazards of working with pathogens make mycobacteria difficult to study and are largely responsible for our poor understanding of these organisms. In this video we will demonstrate the technique of electroporation, which involves subjecting cells to a brief high electrical impulse to allow the entry of DNA. It is the most widely used method for introducing DNA into mycobacterial cells.

Mikobakteriler, Elektroporasyon

High efficiency transformation is a major limitation in the study of mycobacteria. The genus Mycobacterium can be difficult to transform; this is mainly ...

Biyoloji

In utero and ex vivo Electroporation for Gene Expression in Mouse Retinal Ganglion Cells

The retina and its sole output neuron, the retinal ganglion cell (RGC), comprise an excellent model in which to examine biological questions such as cell differentiation, axon guidance, retinotopic organization and synapse formation[1]. One drawback is the inability to efficiently and reliably manipulate gene expression in RGCs in vivo, especially in the otherwise accessible murine visual pathways. Transgenic mice can be used to manipulate gene expression, but this approach is often expensive, time consuming, and can produce unwanted side effects. In chick, in ovo electroporation is used to manipulate gene expression in RGCs for examining retina and RGC development. Although similar electroporation techniques have been developed in neonatal mouse pups[2], adult rats[3], and embryonic murine retinae in vitro[4], none of these strategies allow full characterization of RGC development and axon projections in vivo. To this end, we have developed two applications of electroporation, one in utero and the other ex vivo, to specifically target embryonic murine RGCs[5, 6]. 
With in utero retinal electroporation, we can misexpress or downregulate specific genes in RGCs and follow their axon projections through the visual pathways in vivo, allowing examination of guidance decisions at intermediate targets, such as the optic chiasm, or at target regions, such as the lateral geniculate nucleus. Perturbing gene expression in a subset of RGCs in an otherwise wild-type background facilitates an understanding of gene function throughout the retinal pathway. Additionally, we have developed a companion technique for analyzing RGC axon growth in vitro. We electroporate embryonic heads ex vivo, collect and incubate the whole retina, then prepare explants from these retinae several days later. Retinal explants can be used in a variety of in vitro assays in order to examine the response of electroporated RGC axons to guidance cues or other factors. In sum, this set of techniques enhances our ability to misexpress or downregulate genes in RGCs and should greatly aid studies examining RGC development and axon projections.

In utero and ex vivo Electroporation for Gene Expression in Mouse Retinal Ganglion Cells

Here we present two techniques for manipulating gene expression in murine retinal ganglion cells (RGCs) by in utero and ex vivo electroporation. These techniques enable one to examine how alterations in gene expression affect RGC development, axon guidance, and functional properties.

Fare Retina Ganglion Hücreleri Gen İfadesi utero ve ex vivo Elektroporasyon

The retina and its sole output neuron, the retinal ganglion cell (RGC), comprise an excellent model in which to examine biological questions such as cell ...

DNA Transfection of Mammalian Skeletal Muscles using In Vivo Electroporation

A growing interest in cell biology is to express transgenically modified forms of essential proteins (e.g. fluorescently tagged constructs and/or mutant variants) in order to investigate their endogenous distribution and functional relevance. An interesting approach that has been implemented to fulfill this objective in fully differentiated cells is the in vivo transfection of plasmids by various methods into specific tissues such as liver1, skeletal muscle2,3, and even the brain4. We present here a detailed description of the steps that must be followed in order to efficiently transfect genetic material into fibers of the flexor digitorum brevis (FDB) and interosseus (IO) muscles of adult mice using an in vivo electroporation approach. The experimental parameters have been optimized so as to maximize the number of muscle fibers transfected while minimizing tissue damages that may impair the quality and quantity of the proteins expressed in individual fibers. We have verified that the implementation of the methodology described in this paper results in a high yield of soluble proteins, i.e. EGFP and ECFP3, calpain, FKBP12, &beta;2a-DHPR, etc. ; structural proteins, i.e. minidystrophin and &alpha;-actinin; and membrane proteins, i.e. &alpha;1s-DHPR, RyR1, cardiac Na/Ca2+ exchanger , NaV1.4 Na channel, SERCA1, etc., when applied to FDB, IO and other muscles of mice and rats. The efficient expression of some of these proteins has been verified with biochemical3 and functional evidence5. However, by far the most common confirmatory approach used by us are standard fluorescent microscopy and 2-photon laser scanning microscopy (TPLSM), which permit to identify not only the overall expression, but also the detailed intracellular localization, of fluorescently tagged protein constructs. The method could be equally used to transfect plasmids encoding for the expression of proteins of physiological relevance (as shown here), or for interference RNA (siRNA) aiming to suppress the expression of normally expressed proteins (not tested by us yet). It should be noted that the transfection of FDB and IO muscle fibers is particularly relevant for the investigation of mammalian muscle physiology since fibers enzymatically dissociated from these muscles are currently one of the most suitable models to investigate basic mechanisms of excitability and excitation-contraction coupling under current or voltage clamp conditions2,6-8.

DNA Transfection of Mammalian Skeletal Muscles using In Vivo Electroporation

We describe detailed procedures for the efficient transfection of plasmid DNA into the fibers of foot muscles of live mice using electroporation and the subsequent visualization of protein expression using fluorescence microscopy.

Memeli İskelet Kaslar kullanarak DNA Transfeksiyon In Vivo Elektroporasyon

 A growing interest in cell biology is to express transgenically modified forms of essential proteins (e.g. fluorescently tagged constructs and/or mutant ...

Single-cell Suction Recordings from Mouse Cone Photoreceptors

Rod and cone photoreceptors in the retina are responsible for light detection. In darkness, cyclic nucleotide-gated (CNG) channels in the outer segment are open and allow cations to flow steadily inwards across the membrane, depolarizing the cell. Light exposure triggers the closure of the CNG channels, blocks the inward cation current flow, and thus results in cell hyperpolarization. Based on the polarity of photoreceptors, a suction recording method was developed in 1970s that, unlike the classic patch-clamp technique, does not require penetrating the plasma membrane 1. Drawing the outer segment into a tightly-fitting glass pipette filled with extracellular solution allows recording the current changes in individual cells upon test-flash exposure. However, this well-established "outer-segment-in (OS-in)" suction recording is not suitable for mouse cone recordings, because of the low percentage of cones in the mouse retina (3%) and the difficulties in identifying the cone outer segments. Recently, an inner-segment-in (IS-in) recording configuration was developed to draw the inner segment/nuclear region of the photoreceptor into the recording pipette 2,3. In this video, we will show how to record from individual mouse cone photoresponses using single-cell suction electrode.

We will show how to record flash responses from single mouse cones using a suction electrode.

Tek hücreli fare Koni fotoreseptörlerin Emiş Kayıtlar

Rod and cone photoreceptors in the retina are responsible for light detection. In darkness, cyclic nucleotide-gated (CNG) channels in the outer segment ...

In vivo Imaging of Intact Drosophila Larvae at Sub-cellular Resolution

Recent improvements in optical imaging, genetically encoded fluorophores and genetic tools allowing efficient establishment of desired transgenic animal lines have enabled biological processes to be studied in the context of a living, and in some instances even behaving, organism. In this protocol we will describe how to anesthetize intact Drosophila larvae, using the volatile anesthetic desflurane, to follow the development and plasticity of synaptic populations at sub-cellular resolution1-3. While other useful methods to anesthetize Drosophila melanogaster larvae have been previously described4,5,6,7,8, the protocol presented herein demonstrates significant improvements due to the following combined key features: (1) A very high degree of anesthetization; even the heart beat is arrested allowing for lateral resolution of up to 150 nm1, (2) a high survival rate of &gt; 90% per anesthetization cycle, permitting the recording of more than five time-points over a period of hours to days2 and (3) a high sensitivity enabling us in 2 instances to study the dynamics of proteins expressed at physiological levels. In detail, we were able to visualize the postsynaptic glutamate receptor subunit GluR-IIA expressed via the endogenous promoter1 in stable transgenic lines and the exon trap line FasII-GFP1. (4) In contrast to other methods4,7 the larvae can be imaged not only alive, but also intact (i.e. non-dissected) allowing observation to occur over a number of days1. The accompanying video details the function of individual parts of the in vivo imaging chamber2,3, the correct mounting of the larvae, the anesthetization procedure, how to re-identify specific positions within a larva and the safe removal of the larvae from the imaging chamber.

In vivo Imaging of Intact Drosophila Larvae at Sub-cellular Resolution

This protocol describes a reliable method for anesthetization and imaging of intact Drosophila melanogaster larvae. We have utilized the volatile anesthetic desflurane to allow for repetitive imaging at sub-cellular resolution and re-identification of structures for up to a few days1.

Alt hücresel Çözünürlük bozulmamış Drosophila Larva in vivo Görüntüleme

Recent improvements in optical imaging, genetically encoded fluorophores and genetic tools allowing efficient establishment of desired transgenic animal ...

In vivo Electroporation of Morpholinos into the Adult Zebrafish Retina

Many devastating inherited eye diseases result in progressive and irreversible blindness because humans cannot regenerate dying or diseased retinal neurons. In contrast, the adult zebrafish retina possesses the robust ability to spontaneously regenerate any neuronal class that is lost in a variety of different retinal damage models, including retinal puncture, chemical ablation, concentrated high temperature, and intense light treatment 1-8. Our lab extensively characterized regeneration of photoreceptors following constant intense light treatment and inner retinal neurons after intravitreal ouabain injection 2, 5, 9. In all cases, resident M&uuml;ller glia re-enter the cell cycle to produce neuronal progenitors, which continue to proliferate and migrate to the proper retinal layer, where they differentiate into the deficient neurons. 
	We characterized five different stages during regeneration of the light-damaged retina that were highlighted by specific cellular responses. We identified several differentially expressed genes at each stage of retinal regeneration by mRNA microarray analysis 10. Many of these genes are also critical for ocular development. To test the role of each candidate gene/protein during retinal regeneration, we needed to develop a method to conditionally limit the expression of a candidate protein only at times during regeneration of the adult retina. 
	Morpholino oligos are widely used to study loss of function of specific proteins during the development of zebrafish, Xenopus, chick, mouse, and tumors in human xenografts 11-14. These modified oligos basepair with complementary RNA sequence to either block the splicing or translation of the target RNA. Morpholinos are stable in the cell and can eliminate or "knockdown" protein expression for three to five days 12. 
	Here, we describe a method to efficiently knockdown target protein expression in the adult zebrafish retina. This method employs lissamine-tagged antisense morpholinos that are injected into the vitreous of the adult zebrafish eye. Using electrode forceps, the morpholino is then electroporated into all the cell types of the dorsal and central retina. Lissamine provides the charge on the morpholino for electroporation and can be visualized to assess the presence of the morpholino in the retinal cells. 
	Conditional knockdown in the retina can be used to examine the role of specific proteins at different times during regeneration. Additionally, this approach can be used to study the role of specific proteins in the undamaged retina, in such processes as visual transduction and visual processing in second order neurons.

In vivo Electroporation of Morpholinos into the Adult Zebrafish Retina

A method to conditionally knockdown a target protein&#x2019;s expression in the adult zebrafish retina is described, which involves intravitreally injecting antisense morpholinos and electroporating them into the retina. The resulting protein is knocked down for several days, which allows testing the protein&#x2019;s role in the regenerating or intact retina.

Morpholinos in vivo Elektroporasyon Yetişkin Zebra balığı Retina

Many devastating inherited eye diseases result in progressive and irreversible blindness because humans cannot regenerate dying or diseased retinal ...

In vivo Electroporation of Morpholinos into the Regenerating Adult Zebrafish Tail Fin

Certain species of urodeles and teleost fish can regenerate their tissues. Zebrafish have become a widely used model to study the spontaneous regeneration of adult tissues, such as the heart1, retina2, spinal cord3, optic nerve4, sensory hair cells5, and fins6.
The zebrafish fin is a relatively simple appendage that is easily manipulated to study multiple stages in epimorphic regeneration. Classically, fin regeneration was characterized by three distinct stages: wound healing, blastema formation, and fin outgrowth. After amputating part of the fin, the surrounding epithelium proliferates and migrates over the wound. At 33 &deg;C, this process occurs within six hours post-amputation (hpa, Figure 1B)6,7. Next, underlying cells from different lineages (ex. bone, blood, glia, fibroblast) re-enter the cell cycle to form a proliferative blastema, while the overlying epidermis continues to proliferate (Figure 1D)8. Outgrowth occurs as cells proximal to the blastema re-differentiate into their respective lineages to form new tissue (Figure 1E)8. Depending on the level of the amputation, full regeneration is completed in a week to a month.
The expression of a large number of gene families, including wnt, hox, fgf, msx, retinoic acid, shh, notch, bmp, and activin-betaA genes, is up-regulated during specific stages of fin regeneration9-16. However, the roles of these genes and their encoded proteins during regeneration have been difficult to assess, unless a specific inhibitor for the protein exists13, a temperature-sensitive mutant exists or a transgenic animal (either overexpressing the wild-type protein or a dominant-negative protein) was generated7,12. We developed a reverse genetic technique to quickly and easily test the function of any gene during fin regeneration.
Morpholino oligonucleotides are widely used to study loss of specific proteins during zebrafish, Xenopus, chick, and mouse development17-19. Morpholinos basepair with a complementary RNA sequence to either block pre-mRNA splicing or mRNA translation. We describe a method to efficiently introduce fluorescein-tagged antisense morpholinos into regenerating zebrafish fins to knockdown expression of the target protein. The morpholino is micro-injected into each blastema of the regenerating zebrafish tail fin and electroporated into the surrounding cells. Fluorescein provides the charge to electroporate the morpholino and to visualize the morpholino in the fin tissue.
This protocol permits conditional protein knockdown to examine the role of specific proteins during regenerative fin outgrowth. In the Discussion, we describe how this approach can be adapted to study the role of specific proteins during wound healing or blastema formation, as well as a potential marker of cell migration during blastema formation.

In vivo Electroporation of Morpholinos into the Regenerating Adult Zebrafish Tail Fin

We describe a method to conditionally knockdown the expression of a target protein during adult zebrafish fin regeneration. This technique involves micro-injecting and electroporating antisense oligonucleotide morpholinos into fin tissue, which allows testing the protein&#x2019;s role in various stages of fin regeneration, including wound healing, blastema formation, and regenerative outgrowth.

Yenileyici Yetişkin Zebra balığı Tail Fin içine Morpholinos in vivo olarak Elektroporasyon

Certain species of urodeles and teleost fish can regenerate their tissues. Zebrafish have become a widely used model to study the spontaneous regeneration ...

Confocal Imaging of Single Mitochondrial Superoxide Flashes in Intact Heart or In Vivo

Mitochondrion is a critical intracellular organelle responsible for energy production and intracellular signaling in eukaryotic systems. Mitochondrial dysfunction often accompanies and contributes to human disease. Majority of the approaches that have been developed to evaluate mitochondrial function and dysfunction are based on in vitro or ex vivo measurements. Results from these experiments have limited ability in determining mitochondrial function in vivo. Here, we describe a novel approach that utilizes confocal scanning microscopy for the imaging of intact tissues in live aminals, which allows the evaluation of single mitochondrial function in a real-time manner in vivo. First, we generate transgenic mice expressing the mitochondrial targeted superoxide indicator, circularly permuted yellow fluorescent protein (mt-cpYFP). Anesthetized mt-cpYFP mouse is fixed on a custom-made stage adaptor and time-lapse images are taken from the exposed skeletal muscles of the hindlimb. The mouse is subsequently sacrificed and the heart is set up for Langendorff perfusion with physiological solutions at 37 &deg;C. The perfused heart is positioned in a special chamber on the confocal microscope stage and gentle pressure is applied to immobilize the heart and suppress heart beat induced motion artifact. Superoxide flashes are detected by real-time 2D confocal imaging at a frequency of one frame per second. The perfusion solution can be modified to contain different respiration substrates or other fluorescent indicators. The perfusion can also be adjusted to produce disease models such as ischemia and reperfusion. This technique is a unique approach for determining the function of single mitochondrion in intact tissues and in vivo.

Confocal Imaging of Single Mitochondrial Superoxide Flashes in Intact Heart or In Vivo

Confocal scanning microscopy is applied for imaging single mitochondrial events in perfused heart or skeletal muscles in live animal. Real-time monitoring of single mitochondrial processes such as superoxide flashes and membrane potential fluctuations enables the evaluation of mitochondrial function in a physiologically relevant context and during pathological perturbations.

Tek Mitokondriyal süperoksit Bozulmamış Kalp Flaşlar veya konfokal Görüntüleme<em&gt; In Vivo</em

Mitochondrion is a critical intracellular organelle responsible for energy production and intracellular signaling in eukaryotic systems. Mitochondrial ...

Assessment of Calcium Sparks in Intact Skeletal Muscle Fibers

Maintaining homeostatic Ca2+ signaling is a fundamental physiological process in living cells. Ca2+ sparks are the elementary units of Ca2+ signaling in the striated muscle fibers that appear as highly localized Ca2+ release events mediated by ryanodine receptor (RyR) Ca2+ release channels on the sarcoplasmic reticulum (SR) membrane. Proper assessment of muscle Ca2+ sparks could provide information on the intracellular Ca2+&#160;handling properties of healthy and diseased striated muscles. Although Ca2+ sparks events are commonly seen in resting cardiomyocytes, they are rarely observed in resting skeletal muscle fibers; thus there is a need for methods to generate and analyze sparks in skeletal muscle fibers.
Detailed here is an experimental protocol for measuring Ca2+ sparks in isolated flexor digitorm brevis (FDB) muscle fibers using fluorescent Ca2+ indictors and laser scanning confocal microscopy. In this approach, isolated FDB fibers are exposed to transient hypoosmotic stress followed by a return to isotonic physiological solution. Under these conditions, a robust Ca2+ sparks response is detected adjacent to the sarcolemmal membrane in young healthy FDB muscle fibers. Altered Ca2+ sparks response is detected in dystrophic or aged skeletal muscle fibers. This approach has recently demonstrated that membrane-delimited signaling involving cross-talk between inositol (1,4,5)-triphosphate receptor (IP3R) and RyR contributes to Ca2+ spark activation in skeletal muscle. In summary, our studies using osmotic stress induced Ca2+ sparks showed that this intracellular response reflects a muscle signaling mechanism in physiology and aging/disease states, including mouse models of muscle dystrophy (mdx mice) or amyotrophic lateral sclerosis (ALS model).

Described here is a method to directly measure calcium sparks, the elementary units of Ca2+ release from sarcoplasmic reticulum&#160;in intact skeletal muscle fibers. This method utilizes osmotic-stress-mediated triggering of Ca2+ release from ryanodine receptor in isolated muscle fibers. The dynamics and homeostatic capacity of intracellular Ca2+ signaling can be employed to assess muscle function in health and disease.

Kalsiyum değerlendirilmesi Bozulmamış İskelet kas liflerinin içinde Sparks

Maintaining homeostatic Ca2+ signaling is a fundamental physiological process in living cells. Ca2+ sparks are the elementary units of Ca2+ signaling in ...

In Vivo Microinjection and Electroporation of Mouse Testis

This video and article contribution gives a comprehensive description of microinjection and electroporation of mouse testis in vivo. This particular transfection technique for testicular mouse cells allows the study of unique processes in spermatogenesis.
The following protocol focuses on transfection of testicular mouse cells with plasmid constructs. Specifically, we used the reporter vector pEGFP-C1, which expresses enhanced green fluorescent protein (eGFP) and also the pDsRed2-N1 vector expressing red fluorescent protein (DsRed2). Both encoded reporter genes were under the control of the human cytomegalovirus immediate-early promoter (CMV).
For performing gene transfer into mouse testes, the reporter plasmid constructs are injected into testes of living mice. To that end, the testis of an anaesthetized animal is exposed and the site of microinjection is prepared. Our preferred place of injection is the efferent duct, with the ultimately connected rete testis as the anatomical transport route of the spermatozoa between the testis and the epididymis. In this way, the filling of the seminiferous tubules after microinjection is excellently managed and controlled due to the use of stained DNA solutions. After observing a sufficient filling of the testis by its colored tubule structure, the organ is electroporated. This enables the transfer of the DNA solution into the testicular&#160;cells. Following 3 days of incubation, the testis is removed and investigated under the microscope for green or red&#160;fluorescence, illustrating transfection success.
Generally, this protocol can be employed for delivering DNA- or RNA- constructs into living mouse testis in order to (over)express or knock down genes, facilitating in vivo gene function analysis. Furthermore, it is suitable for studying reporter constructs or putative gene regulatory elements. Thus, the main advantages of the electroporation technique are fast performance in combination with low effort as well as the moderate technical equipment and skills required compared to alternative techniques.

In Vivo Microinjection and Electroporation of Mouse Testis

This article describes microinjection and electroporation of mouse testis in&#160;vivo as a&#160;transfection technique for testicular mouse cells to study unique processes of spermatogenesis. The presented protocol involves steps of glass capillary preparation, microinjection via the efferent duct, and transfection by electroporation.

Fare Testis İn Vivo Mikroenjeksiyon ve Elektroporasyon

This video and article contribution gives a comprehensive description of microinjection and electroporation of mouse testis in vivo. This particular ...