パッチクランプの設定： 光学系：良いセルを見つけるために、そしてそれの位置を確立するために光学系は非常に重要である。 鋭いエッジ、柔らかそうに見えるセル：セルのクリアな画像を取得してください。 添付の萼との良好なMNTB主細胞を探すためにフィールド全体をスキャンします。別の角度から腎杯を探すために皿を回転させる。最初は、それは風船の形をした端末上で練習するOKです。 スライスの表面にあるセルを選択、または第2の細胞層に。ピペットで細胞の最初の1 / 3 回を対象と がくの識別：（図1を参照）二重膜を探して、そしてそれが萼であることを確認するためのさまざまな角度からそれを見るためにスライス皿を回転させる。 <img src="/files/ftp_upload/old/244_2008_8_22_2/244_Figure-01.png" alt="図1" width="298" height="159" /> 図1 がくの深さ：がくが表面上にあるか、できるだけ表面に近いはず。 パッチ適用に使用できる表面：判断するために顕微鏡で使用して微フォーカスノブ方法&quot;深さ/幅の&quot;がくです。例えば、ファインフォーカスのフルターン〜10％があなたの上にパッチを適用するのに十分な表面積よりも多くを与える。 シナプス前細胞の上にシール：アタッチされたセルを取得するには、ピペットのposの圧力（〜0.15psi）による細胞表面上に&quot;小さな&quot;変形を探して、ダウンして全体で、ピペットを実行するためのマニピュレータを使用して、とさえへ必要に応じてとのような良好な変形を得るためにpresyn端子の表面には、その後、圧力を解放し、吸引を適用します。 PULSE、データ取得プログラム： 最初に使用する前にバッファサイズを増やす必要がある、とするたびに容量をサンプリングすることによって必要。 修正されたマクロたびにロードする必要があります。 液体ジャンクショ​​ンポテンシャルPresyn録音ソリューションは、（11mV負）- 11mVです。 Presyn：Cslow =〜15 pFの presyn用のRSカンプ：10マイクロ秒、65％（以上補償可能性のあるW /外振動） 記録容量の前に：テスト現在のリラクゼーション（10 mVの、10ミリ秒のジャンプが）緩和がmonoexponentialであるかどうかを確認するために、すなわち、presynの用語は、単一の区画でモデル化できるかどうか。 フィルタ：高速なコンポーネントが上を逃したしていないことを確認するため、緩和測定中に30 kHzと10 kHz（各ベッセルフィルタ1と2）で設定します。 ミニ録音中に、新生は10 kHzと5kHzのを使用。 LGWは、我々はミニの立ち上がり時間を測定することができることを確認するために30 kHzでのみフィルター1セットを使用するように私に尋ねた。 ファイル命名規則：7桁のmmは月000mmxx、（または月と年）とxxはセル番号です。 ソリューションラインを清掃：0.1 M塩酸20 mlの実験の終了時にクリーンアップラインズは、200ミリリットルddH2Oが続きます。 外部ソリューションがリサイクルされ 、ポンプの速度は、20〜30 rpmです。 （入浴室から戻って解決策は、メスシリンダーに逆流）。 十分な吸引を確保するために3の発信回線を設定します。 ピペットシナプス前レコーディングソリューション：〜310ミリ浸透圧 Presynソリューションは、実験中にR -アクセスの増加を防ぐために〜310 mOsmである必要があります。 Presynピペット溶液はpostsynピペット溶液（PresynはEXのATPとGTPを持っている。）とは異なります。 TTX - TEA溶液（カルシウム電流を単離すること）： <ul><li>ソリューションのブロックK -チャネルにおけるTEAとして、セルの上に、シール、あるいはパッチ適用後に適用しようと細胞を脱分極。これは、細胞にとって好ましいことではありません。同じ理由で、それは、TTXが適用された後に、スライスを再利用できないことがあります。 </li><li>セル、または持続性脱分極の影響を確認するためにスライスの最初と最後の応答を比較する。 </li><li>効果が速くなるように、TTXは1μMの代わりに0.5μMで使用されています。ソリューションを変更した後、短い時間を待機する必要があります。 </li></ul>切断スライスビブラトームの設定： <ul><li> 70Hzの横振動</li><li>振幅：1.0ミリメートル</li><li>萼で、スライスをカットしながら前進、0.1以外の場合厚さ0.01〜0.02ミリメートル/秒のスピード：180μmのを（〜150高齢動物の程度） </li></ul>スライスは、1時間（カット時間を含む）、すなわち、15〜20分切削後のお風呂に残すために37℃でインキュベートする。 ピペット： Presyn：最初MΩ3.5から4.5、3.0から3.5MΩもっと自信設定値を設定するには、引き手のマニュアルを使用してください。ガラスが厚いため、遅延機能を使用します（200または1作業の遅延） ガラスのタイプ：ホウケイ酸、標準の壁、無フィラメント外径：2.0ミリメートル内径1.16ミリメートル長さ：7.5センチメートル

methods for patch clamp capacitance recordings from the calyx

私たちは、開催のがくにおけるシナプス前のパッチクランプ記録、哺乳類の中枢神経系の神経終末のための基本的な手法を示します。シナプス前終末からの電気の録音は、活動電位、カルシウムチャネル電流、小胞融合（エキソサイトーシス）と、その後の膜の取り込み（エンドサイトーシス）の測定を可能にする。神経伝達物質を含む小胞の融合は、小胞膜ががくの細胞膜に追加されます。細胞膜の量のこの増加は、容量の増加として測定されます。静電容量で、その後の減少は、エンドサイトーシス、萼の膜から細胞膜への取り込みや削除のプロセスを示している。エンドサイトーシスは、がくの構造を維持するために必要であり、それはまた将来のエキソサイトーシスのイベントのための神経伝達物質で満たされる小胞を形成する必要がある。ハンドヘルドのがくでの容量の記録により、直接、急速に小胞放出と哺乳類の中枢神経系の神経終末の後続のエンドサイトーシスを測定するために作られている。さらに、対応する後シナプス活性が同時にペアの録音を使用して測定することができます。したがって、中枢神経系のシナプスにおけるシナプス前及びシナプス後の電気的活動の全体像は、この準備を用いて達成可能です。ここでは、スライスの準備、開催される基本的なパッチクランプ技術の腎杯の識別のための形態学的特徴、及びエキソサイトーシスとエンドサイトーシスを測定する静電容量の記録の例のための方法が提示されます。

Watch this Scientific Journal Video about Methods for Patch Clamp Capacitance Recordings from the Calyx at JoVE.com

Methods for Patch Clamp Capacitance Recordings from the Calyx

がくからパッチクランプの静電容量の録音のための方法

We demonstrate the basic techniques for presynaptic patch clamp recording at the calyx of Held, a mammalian central nervous system nerve terminal. ...

methods-for-patch-clamp-capacitance-recordings-from-the-calyx

Research

JoVE Journal

Biology

12.6K ビュー.  National Institute of Health. 

ビデオ: Methods for Patch Clamp Capacitance Recordings from the Calyx

Patch Clamp Recording of Ion Channels Expressed in  Xenopus Oocytes

Since its development by Sakmann and Neher 1, 2, the patch clamp has become established as an extremely useful technique for electrophysiological measurement of single or multiple ion channels in cells. This technique can be applied to ion channels in both their native environment and expressed in heterologous cells, such as oocytes harvested from the African clawed frog, Xenopus laevis. Here, we describe the well-established technique of patch clamp recording from Xenopus oocytes. This technique is used to measure the properties of expressed ion channels either in populations (macropatch) or individually (single-channel recording). We focus on techniques to maximize the quality of oocyte preparation and seal generation. With all factors optimized, this technique gives a probability of successful seal generation over 90 percent. The process may be optimized differently by every researcher based on the factors he or she finds most important, and we present the approach that have lead to the greatest success in our hands.

This is intended as an introduction to patch clamp recording from Xenopus laevis oocytes. It covers vitelline membrane removal, formation of a gigaohm seal (gigaseal), and the optional conversion of the patch to the outside-out topology.

アフリカツメガエルの卵母細胞で発現イオンチャネルのパッチクランプ記録

Since its development by Sakmann and Neher 1, 2, the patch clamp has become established as an extremely useful technique for electrophysiological ...

生物学

Pressure-polishing Pipettes for Improved Patch-clamp Recording

Pressure-polishing is a method for shaping glass pipettes for patch-clamp recording. We first developed this method for fabricating pipettes suitable for recording from small (&lt;3 m) neuronal cell bodies. The basic principal is similar to glass-blowing and combines air pressure and heat to modify the shape of patch pipettes prepared by a conventional micropipette puller. It can be applied to so-called soft (soda lime) and hard (borosilicate) glasses. Generally speaking, pressure polishing can reduce pipette resistance by 25% without decreasing the diameter of the tip opening (Goodman and Lockery, 2000). It can be applied to virtually any type of glass and requires only the addition of a high-pressure valve and fitting to a microforge. This technique is essential for recording from ultrasmall cells (&lt;5 m) and can also improve single-channel recording by minimizing pipette resistance. The blunt shape is also useful for perforated-patch clamp recording since this tip shape results in a larger membrane bleb available for perforation.

This is a guide to modifying the shape of glass micropipettes. Specifically, by using heat and air pressure the taper is widened without increasing the tip opening, leading to lower pipette resistance. This is critical to obtain low noise recordings of small cells but is useful in many applications.

改善されたパッチクランプ記録のための圧力 - 研磨ピペット

Pressure-polishing is a method for shaping glass pipettes for patch-clamp recording.  We first developed this method for fabricating pipettes suitable for ...

Electrophysiological Methods for Recording Synaptic Potentials from the NMJ of Drosophila Larvae

In this video, we describe the electrophysiological methods for recording synaptic transmission at the neuromuscular junction (NMJ) of Drosophila larva. The larval neuromuscular system is a model synapse for the study of synaptic physiology and neurotransmission, and is a valuable research tool that has defined genetics and is accessible to experimental manipulation. Larvae can be dissected to expose the body wall musculature, central nervous system, and peripheral nerves. The muscles of Drosophila and their innervation pattern are well characterized and muscles are easy to access for intracellular recording. Individual muscles can be identified by their location and orientation within the 8 abdominal segments, each with 30 muscles arranged in a pattern that is repeated in segments A2 - A7. Dissected drosophila larvae are thin and individual muscles and bundles of motor neuron axons can be visualized by transillumination1. Transgenic constructs can be used to label target cells for visual identification or for manipulating gene products in specific tissues. In larvae, excitatory junction potentials (EJP&#8217;s) are generated in response to vesicular release of glutamate from the motoneurons at the synapse. In dissected larvae, the EJP can be recorded in the muscle with an intracellular electrode. Action potentials can be artificially evoked in motor neurons that have been cut posterior to the ventral ganglion, drawn into a glass pipette by gentle suction and stimulated with an electrode. These motor neurons have distinct firing thresholds when stimulated, and when they fire simultaneously, they generate a response in the muscle. Signals transmitted across the NMJ synapse can be recorded in the muscles that the motor neurons innervate. The EJP&#8217;s and minature excitatory junction potentials (mEJP&#8217;s) are seen as changes in membrane potential. Electrophysiological responses are recorded at room temperature in modified minimal hemolymph-like solution2 (HL3) that contains 5 mM Mg2+ and 1.5 mM Ca2+. Changes in the amplitude of evoked EJP&#8217;s can indicate differences in synaptic function and structure. Digitized recordings are analyzed for EJP amplitude, mEJP frequency and amplitude, and quantal content.

Here we describe electrophysiological methods for measuring synaptic transmission at the neuromuscular junction of Drosophila larva. Evoked release is initiated artificially by stimulating the motor neuron axons, and transmission through the NMJ can be measured by the postsynaptic response evoked in the muscle.

ショウジョウバエの幼虫のNMJからシナプス電位を記録するための電気生理学的方法

In this video, we describe the electrophysiological methods for recording synaptic transmission at the neuromuscular junction (NMJ) of Drosophila larva. ...

Patch Clamp and Perfusion Techniques for Studying Ion Channels Expressed in Xenopus oocytes

The protocol presented here is designed to study the activation of the large conductance, voltage- and Ca2+-activated K+ (BK) channels. The protocol may also be used to study the structure-function relationship for other ion channels and neurotransmitter receptors1. BK channels are widely expressed in different tissues and have been implicated in many physiological functions, including regulation of smooth muscle contraction, frequency tuning of inner hair cells and regulation of neurotransmitter release2-6. BK channels are activated by membrane depolarization and by intracellular Ca2+ and Mg2+ 6-9. Therefore, the protocol is designed to control both the membrane voltage and the intracellular solution. In this protocol, messenger RNA of BK channels is injected into Xenopus laevis oocytes (stage V-VI) followed by 2-5 days of incubation at 18&deg;C10-13. Membrane patches that contain single or multiple BK channels are excised with the inside-out configuration using patch clamp techniques10-13. The intracellular side of the patch is perfused with desired solutions during recording so that the channel activation under different conditions can be examined. To summarize, the mRNA of BK channels is injected into Xenopus laevis oocytes to express channel proteins on the oocyte membrane; patch clamp techniques are used to record currents flowing through the channels under controlled voltage and intracellular solutions.

Patch Clamp and Perfusion Techniques for Studying Ion Channels Expressed in Xenopus oocytes

Ionic current of BK channels is recorded using patch clamp techniques. BK channels are expressed in Xenopus oocytes by injecting messenger RNA. The intracellular solution during patch clamp recordings is controlled by a perfusion system.

イオンチャネル研究のためのパッチクランプおよび灌流のテクニックで表さアフリカツメガエル卵母細胞

The protocol presented here is designed to study the activation of the large conductance, voltage- and Ca2+-activated K+ (BK) channels. The protocol may ...

Exploring Arterial Smooth Muscle Kv7 Potassium Channel Function using Patch Clamp Electrophysiology and Pressure Myography

Contraction or relaxation of smooth muscle cells within the walls of resistance arteries determines the artery diameter and thereby controls flow of blood through the vessel and contributes to systemic blood pressure. The contraction process is regulated primarily by cytosolic calcium concentration ([Ca2+]cyt), which is in turn controlled by a variety of ion transporters and channels. Ion channels are common intermediates in signal transduction pathways activated by vasoactive hormones to effect vasoconstriction or vasodilation. And ion channels are often targeted by therapeutic agents either intentionally (e.g. calcium channel blockers used to induce vasodilation and lower blood pressure) or unintentionally (e.g. to induce unwanted cardiovascular side effects).
Kv7 (KCNQ) voltage-activated potassium channels have recently been implicated as important physiological and therapeutic targets for regulation of smooth muscle contraction. To elucidate the specific roles of Kv7 channels in both physiological signal transduction and in the actions of therapeutic agents, we need to study how their activity is modulated at the cellular level as well as evaluate their contribution in the context of the intact artery.
The rat mesenteric arteries provide a useful model system. The arteries can be easily dissected, cleaned of connective tissue, and used to prepare isolated arterial myocytes for patch clamp electrophysiology, or cannulated and pressurized for measurements of vasoconstrictor/vasodilator responses under relatively physiological conditions. Here we describe the methods used for both types of measurements and provide some examples of how the experimental design can be integrated to provide a clearer understanding of the roles of these ion channels in the regulation of vascular tone.

Measurements of Kv7 (KCNQ) potassium channel activity in isolated arterial myocytes (using patch clamp electrophysiological techniques) in parallel with measurements of constrictor/dilator responses (using pressure myography) can reveal important information about the roles of Kv7 channels in vascular smooth muscle physiology and pharmacology.

パッチクランプ電気生理学および圧力筋運動記録法を用いた動脈平滑筋KV7カリウムチャネル機能を探る

Contraction  or relaxation of smooth muscle cells within the walls of resistance arteries  determines the artery diameter and thereby controls flow of ...

Giant Liposome Preparation for Imaging and Patch-Clamp Electrophysiology

The reconstitution of ion channels into chemically defined lipid membranes for electrophysiological recording has been a powerful technique to identify and explore the function of these important proteins. However, classical preparations, such as planar bilayers, limit the manipulations and experiments that can be performed on the reconstituted channel and its membrane environment. The more cell-like structure of giant liposomes permits traditional patch-clamp experiments without sacrificing control of the lipid environment.
Electroformation is an efficient mean to produce giant liposomes &gt;10 &mu;m in diameter which relies on the application of alternating voltage to a thin, ordered lipid film deposited on an electrode surface. However, since the classical protocol calls for the lipids to be deposited from organic solvents, it is not compatible with less robust membrane proteins like ion channels and must be modified. Recently, protocols have been developed to electroform giant liposomes from partially dehydrated small liposomes, which we have adapted to protein-containing liposomes in our laboratory.
We present here the background, equipment, techniques, and pitfalls of electroformation of giant liposomes from small liposome dispersions. We begin with the classic protocol, which should be mastered first before attempting the more challenging protocols that follow. We demonstrate the process of controlled partial dehydration of small liposomes using vapor equilibrium with saturated salt solutions. Finally, we demonstrate the process of electroformation itself. We will describe simple, inexpensive equipment that can be made in-house to produce high-quality liposomes, and describe visual inspection of the preparation at each stage to ensure the best results.

Reconstituting functional membrane proteins into giant liposomes of defined composition is a powerful approach when combined with patch-clamp electrophysiology. However, conventional giant liposome production may be incompatible with protein stability. We describe protocols for producing giant liposomes from pure lipids or small liposomes containing ion channels.

イメージングとパッチクランプ電気生理学用ジャイアントリポソーム製剤

The reconstitution of ion channels into chemically defined lipid membranes for electrophysiological recording has been a powerful technique to identify ...

One-channel Cell-attached Patch-clamp Recording

Ion channel proteins are universal devices for fast communication across biological membranes. The temporal signature of the ionic flux they generate depends on properties intrinsic to each channel protein as well as the mechanism by which it is generated and controlled and represents an important area of current research. Information about the operational dynamics of ion channel proteins can be obtained by observing long stretches of current produced by a single molecule. Described here is a protocol for obtaining one-channel cell-attached patch-clamp current recordings for a ligand gated ion channel, the NMDA receptor, expressed heterologously in HEK293 cells or natively in cortical neurons. Also provided are instructions on how to adapt the method to other ion channels of interest by presenting the example of the mechano-sensitive channel PIEZO1. This method can provide data regarding the channel&#8217;s conductance properties and the temporal sequence of open-closed conformations that make up the channel&#8217;s activation mechanism, thus helping to understand their functions in health and disease.

Described here is a procedure for obtaining long stretches of current recording from one ion channel with the cell-attached patch-clamp technique. This method allows for observing, in real time, the pattern of open-close channel conformations that underlie the biological signal. These data inform about channel properties in undisturbed biological membranes.

一チャネルセル付パッチクランプ法

Ion channel proteins are universal devices for fast communication across biological membranes. The temporal signature of the ionic flux they generate ...

Reconstitution of a Transmembrane Protein, the Voltage-gated Ion Channel, KvAP, into Giant Unilamellar Vesicles for Microscopy and Patch Clamp Studies

Giant Unilamellar Vesicles (GUVs) are a popular biomimetic system for studying membrane associated phenomena. However, commonly used protocols to grow GUVs must be modified in order to form GUVs containing functional transmembrane proteins. This article describes two dehydration-rehydration methods &#8212; electroformation and gel-assisted swelling &#8212; to form GUVs containing the voltage-gated potassium channel, KvAP. In both methods, a solution of protein-containing small unilamellar vesicles is partially dehydrated to form a stack of membranes, which is then allowed to swell in a rehydration buffer. For the electroformation method, the film is deposited on platinum electrodes so that an AC field can be applied during film rehydration. In contrast, the gel-assisted swelling method uses an agarose gel substrate to enhance film rehydration. Both methods can produce GUVs in low (e.g., 5 mM) and physiological (e.g., 100 mM) salt concentrations. The resulting GUVs are characterized via fluorescence microscopy, and the function of reconstituted channels measured using the inside-out patch-clamp configuration. While swelling in the presence of an alternating electric field (electroformation) gives a high yield of defect-free GUVs, the gel-assisted swelling method produces a more homogeneous protein distribution and requires no special equipment.

The reconstitution of the transmembrane protein, KvAP, into giant unilamellar vesicles (GUVs) is demonstrated for two dehydration-rehydration methods &#8212; electroformation, and gel-assisted swelling. In both methods, small unilamellar vesicles containing the protein are fused together to form GUVs that can then be studied by fluorescence microscopy and patch-clamp electrophysiology.

膜貫通タンパク質の再構成、顕微鏡およびパッチクランプ研究のための巨大単膜小胞への電位依存性イオンチャネル、KvAP、

Giant Unilamellar Vesicles (GUVs) are a popular biomimetic system for studying membrane associated phenomena. However, commonly used protocols to grow ...

Implementing Patch Clamp and Live Fluorescence Microscopy to Monitor Functional Properties of Freshly Isolated PKD Epithelium

Cyst initiation and expansion during polycystic kidney disease is a complex process characterized by abnormalities in tubular cell proliferation, luminal fluid accumulation and extracellular matrix formation. Activity of ion channels and intracellular calcium signaling are key physiologic parameters which determine functions of tubular epithelium. We developed a method suitable for real-time observation of ion channels activity with patch-clamp technique and registration of intracellular Ca2+ level in epithelial monolayers freshly isolated from renal cysts. PCK rats, a genetic model of autosomal recessive polycystic kidney disease (ARPKD), were used here for ex vivo analysis of ion channels and calcium flux. Described here is a detailed step-by-step procedure designed to isolate cystic monolayers and non-dilated tubules from PCK or normal Sprague Dawley (SD) rats, and monitor single channel activity and intracellular Ca2+ dynamics. This method does not require enzymatic processing and allows analysis in a native setting of freshly isolated epithelial monolayer. Moreover, this technique is very sensitive to intracellular calcium changes and generates high resolution images for precise measurements. Finally, isolated cystic epithelium can be further used for staining with antibodies or dyes, preparation of primary cultures and purification for various biochemical assays.

Ion channels expressed in renal tubular epithelium play a significant role in the pathology of polycystic kidney disease. Here we describe experimental protocols used to perform patch-clamp analysis and intracellular calcium level measurements in cystic epithelium freshly isolated from rodent kidneys.

新たに単離したPKD上皮の機能的特性を監視するためにパッチクランプし、ライブ蛍光顕微鏡を実装

Cyst initiation and expansion during polycystic kidney disease is a complex process characterized by abnormalities in tubular cell proliferation, luminal ...

Methods for the Isolation, Culture, and Functional Characterization of Sinoatrial Node Myocytes from Adult Mice

Sinoatrial node myocytes (SAMs) act as the natural pacemakers of the heart, initiating each heart beat by generating spontaneous action potentials (APs). These pacemaker APs reflect the coordinated activity of numerous membrane currents and intracellular calcium cycling. However the precise mechanisms that drive spontaneous pacemaker activity in SAMs remain elusive. Acutely isolated SAMs are an essential preparation for experiments to dissect the molecular basis of cardiac pacemaking. However, the indistinct anatomy, complex microdissection, and finicky enzymatic digestion conditions have prevented widespread use of acutely isolated SAMs. In addition, methods were not available until recently to permit longer-term culture of SAMs for protein expression studies. Here we provide a step-by-step protocol and video demonstration for the isolation of SAMs from adult mice. A method is also demonstrated for maintaining adult mouse SAMs in vitro and for expression of exogenous proteins via adenoviral infection. Acutely isolated and cultured SAMs prepared via these methods are suitable for a variety of electrophysiological and imaging studies.

Methods are demonstrated for the isolation of sinoatrial node myocytes (SAMs) from adult mice for patch clamp electrophysiology or imaging studies. Isolated cells can be used directly or can be maintained in culture to permit expression of proteins of interest, such as genetically encoded reporters.

成体マウスから洞房結節筋細胞の単離、培養、および機能解析のための方法

Sinoatrial node myocytes (SAMs) act as the natural pacemakers of the heart, initiating each heart beat by generating spontaneous action potentials (APs). ...