Name: Isolation of Human Atrial Myocytes for Simultaneous Measurements of Ca2+ Transients and Membrane Currents (Video) | JoVE Journal
Uploaded: 2013-07-03T12:00:00.000+00:00
Duration: 10 min 53 s
Description: Learn to isolate human atrial myocytes for simultaneous measurements of calcium transients and membrane currents using enzymatic digestion and patch clamp techniques. This method advances cardiac disease research.

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5 minutes

In addition, we thank the cardiac surgeons at Heidelberg University for the provision of human atrial tissue and Claudia Liebetrau, Katrin Kupser and Ramona Nagel for their excellent technical support. Special thanks also to Andy W. Trafford for his helpful suggestions and advice during the establishment of the Ca2+ transient measurements. The authors wish to express their deepest gratitude to the members of the Department of Pharmacology and Toxicology (head: Ursula Ravens) of the Dresden University of Technology for the opportunity they offered us to learn basic techniques and skills in cellular electrophysiology and cardiomyocyte isolation.
The authors' research is supported by the German Research Foundation (Do769/1-1-3), the German Federal Ministry of Education and Research through the Atrial Fibrillation Competence Network (01Gi0204) and the German Centre for Cardiovascular Research, the European Union through the European Network for Translational Research in Atrial Fibrillation (EUTRAF, FP7-HEALTH-2010, large-scale integrating project, Proposal No. 261057) and the European-North American Atrial Fibrillation Research Alliance (ENAFRA) grant of Fondation Leducq (07CVD03).
The schematic overview shown in the video file was produced using Servier medical art.

Experimental protocols need to be approved by the local ethics committee and all patients need to give written informed consent. Our research was approved by the ethics committee of the Medical Faculty Mannheim, University of Heidelberg (#2011-216N-MA) and was performed in compliance with all institutional, national and international guidelines for human welfare. All patients gave written informed consent.
0. Obtaining Human Atrial Tissue
During routine cannulation procedures in patients undergoing open-heart surgery for cardiopulmonary bypass grafting, the tip of the right atrial appendage is usually removed and can be used for isolation of atrial cardiomyocytes. After excision the tissue sample is transferred immediately into a 50 ml Falcon tube with sterile Ca2+-free transport solution containing 2,3-butanedione monoxime (Table I; BDM, contractile inhibitor, preventing myocyte contracture). With transport times between 30 and 45 min, we did not recognize a clear advantage of cooling or oxygenation with respect to both number and quality of isolated atrial cardiomyocytes. In general transport to the lab should be as quick as possible. However, if longer transportation time cannot be avoided, transport at 4 °C in oxygenated solution might be advantageous.
1. Prearrangements
<ol>
	<li>Switch on the thermocirculator, which controls the temperature of the jacketed beaker (Table II). Make sure the temperature within the beaker equals 37 °C. Cover the beaker with a glass lid to maintain a constant temperature within the beaker throughout the whole isolation process.</li>
	<li>Weigh the Collagenase I and Protease XXIV into three glass beakers and store it at room temperature. The enzymes will be diluted just before use.</li>
	<li>Store 20 ml of Ca2+ free solution in a Petri dish at 4 °C.</li>
	<li>Store 250 ml of Ca2+ free solution in a water bath at 37 °C.</li>
</ol>
2. Cleaning of the Tissue
<ol>
	<li>Transfer the tissue sample together with the transport solution into a Petri dish (~10 cm diameter) and remove fatty tissue roughly using scissors.</li>
	<li>Weigh the tissue sample. Between 200 and 600 mg are used for cell isolation. The remaining tissue can be frozen in liquid nitrogen for later biochemical analysis.</li>
	<li>Transfer the tissue sample into the Petri dish containing 20 ml Ca2+ free solution at 4 °C (see step 1.3) and chop the tissue sample into small chunks of approximately 1 mm3 in size.</li>
	<li>The following steps should be executed at 37 °C and under continuous gassing with 100% O2. A pipette tip can be placed onto the oxygen tube to avoid strong bubbling and generate continuous air flow.</li>
	<li>Transfer the tissue chunks together with the Ca2+-free solution into the jacketed beaker and stir carefully for about 3 min with a magnetic stirring bar.</li>
	<li>Stop stirring and allow the tissue chunks to settle down for a few seconds. Carefully strain the supernatant through a nylon mesh (200 μm, Table II). Return the restrained tissue chunks from the mesh into the beaker using forceps.</li>
	<li>Refill the beaker with Ca2+ free solution and repeat the washing step 2.4 and 2.5 two times.</li>
</ol>
3. First Enzymatic Digestion
<ol>
	<li>Re-suspend the tissue chunks with 20 ml Enzyme solution E1 (Table I) containing collagenase and protease and stir carefully for 10 min.</li>
	<li>Add 40 μl of 10 mM CaCl2-solution to obtain a final concentration of 20 μM Ca2+.</li>
	<li>After 35 min strain the supernatant carefully through a nylon mesh (200 μm, Table II) in a way that most of the tissue chunks remain in the beaker. Return restrained tissue chunks from the mesh into the beaker.</li>
</ol>
4. Second Enzymatic Digestion
<ol>
	<li>Resuspend the tissue chunks again with 20 ml enzyme solution E2 containing collagenase I only (Table I). Add 40 μl of 10 mM CaCl2-solution immediately to obtain a final concentration of 20 μM Ca2+.</li>
	<li>During the second digestion use scissors to further chop tissue clots occasionally.</li>
	<li>After 5 min take a sample using a Pasteur pipette to check the dissociation of cells. Repeat this every 2-3 min until rod-shaped, striated cardiomyocytes appear.</li>
	<li>Stop stirring and allow the tissue chunks to settle down for about 20-30 sec.</li>
	<li>Strain the supernatant carefully through a nylon mesh (200 μm, Table II) into a 50 ml Falcon tube (Tube A). Return the restrained tissue chunks from the mesh into the beaker.</li>
	<li>Re-suspend the tissue chunks in the beaker with 20 ml storage solution (Table I)10 and further dissociate the cells by gentle mechanical trituration using a 20 ml serological pipette with dispenser. Try to avoid bubble formation since bubbles are detrimental to cell survival and quality.</li>
	<li>Strain the supernatant carefully through a nylon mesh (200 μm, Table II) into a 50 ml Falcon Tube (Tube B).</li>
</ol>
5. Final Preparation and Adjustment of Final Ca2+ Concentration
<ol>
	<li>Centrifuge both Falcon tubes A and B (see step 4.5 and 4.7) at 95 x g for 10 min.</li>
	<li>Remove the supernatant from both tubes carefully by aspiration. Make sure not to disturb the pellet. Discard the supernatant.</li>
	<li>Re-suspend both pellets in 1.5 ml storage solution (Table I) each (room temperature).</li>
	<li>Add two times 7.5 μl of 10 mM CaCl2 solution to each Falcon and stir carefully. Incubate for 10 min after each step.</li>
	<li>Add 15 μl of 10 mM CaCl2 solution to obtain a final Ca2+ concentration of 0.2 mM.</li>
</ol>
6. Loading of Myocytes with the Fluorescent Ca2+-indicator Fluo-3 AM (Figure 1)
<ol>
	<li>Transfer 1.5 ml of cell suspension (tube A and/or tube B) into a 2 ml microcentrifuge tube (Eppendorf tube).</li>
	<li>The following steps should be executed under consideration of the light sensitivity of the fluorescent Ca2+ Indicator Fluo-3.</li>
	<li>Dissolve 50 μg of the membrane permeable acetoxymethyl ester derivative of Fluo-3 (Fluo-3 AM, Table III) in 44 μl of the Pluronic F-127 (Table III) stock solution (20% w/v in anhydrous DMSO) to get a 1 mM Fluo-3 AM stock solution, which can be stored at -20 °C for at most 1 week.</li>
	<li>Add 15 μl of the Fluo-3 AM stock solution to the microcentrifuge tube containing 1.5 ml of cell suspension (see step 6.1) and agitate carefully.</li>
	<li>Incubate the cell suspension for 10 min in an optically opaque box.</li>
	<li>Briefly centrifuge at about 6,000 rpm.</li>
	<li>Discard the supernatant and re-suspend the pellet in 1.5 ml bath solution (Table IV).</li>
	<li>Leave the cell suspension for about 30 min for de-esterification before beginning with experiments.</li>
</ol>
7. Simultaneous Patch-clamp and Epifluorescent Ca2+ Measurements
Since patch-clamp measurements are not the major topic of this review, we refer the interested reader to other publications providing a more in depth description of this technique.11-14 For the sake of completeness we provide a brief summary of a protocol to measure action potentials or L-type Ca2+ currents, both together with simultaneous Ca2+-transient recordings.
During experiments myocytes are superfused at 37 °C with bath solution (Table IV) using a rapid perfusion system (Octaflow IITM, ALA Scientific Instruments, NY). For voltage-clamp experiments, K+ currents are blocked by adding 4-aminopyridine (5 mmol/L) and BaCl2 (0.1 mmol/L) to the bath solution. Borosilicate glass microelectrodes are used and should have tip resistances of 2-5 MΩ when filled with pipette solution (Table V). In addition to the Fluo-3 AM loading of the myocytes (see step 6), Fluo-3 is also included in the pipette solution (Table V). Fluorescence is excited at 488 nm and emitted light (&lt;520 nm) converted to [Ca2+]i assuming
<img alt="Calcium concentration equation diagram; formula: [Ca2+]i=kd(F/Fmax−F); biochemical analysis." fo:content-width="1.540in" fo:src="/files/ftp_upload/50235/50235eq1highres.jpg" src="/files/ftp_upload/50235/50235eq1.jpg" data-altupdatedat="1787630408000" data-alt="Equation 1">
 
where kd=dissociation constant of Fluo-3 (864 nM), F=Fluo-3 fluorescence; Fmax=Ca2+-saturated fluorescence obtained at the end of each experiment.12 Both electrical signals and epifluorescent Ca2+ signals are recorded simultaneously. Action potentials are stimulated at 0.5 Hz in current-clamp mode using 1 msec current pulses of 1.2x threshold strength. L-type Ca2+-currents are measured in voltage-clamp mode using a holding potential of -80 mV and a 100-msec ramp-pulse to -40 mV to inactivate the fast Na+-current, followed by a 100-msec test-pulse to +10 mV at 0.5 Hz.

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<li>Dobrev, D., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Molecular+basis+of+downregulation+of+G-protein-coupled+inward+rectifying+K%2B+current+IK%2CACh+in+chronic+human+atrial+fibrillation%3A+decrease+in+GIRK4+mRNA+correlates+with+reduced+IK%2CACh+and+muscarinic+receptor-mediated+shortening+of+action+potentials%5BTitle%5D)+AND+%22Circulation%22%5BJournal%5D)">Molecular basis of downregulation of G-protein-coupled inward rectifying K+ current IK,ACh in chronic human atrial fibrillation: decrease in GIRK4 mRNA correlates with reduced IK,ACh and muscarinic receptor-mediated shortening of action potentials.</a> Circulation. 104, 2551-2557 (2001).</li>
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</ol>

Worthington Biochemical Corp. supported this publication by covering production costs of video file. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Here we describe a method for isolation of human atrial myocytes from right atrial appendages obtained from patients undergoing open heart surgery. In order to use these myocytes for measurements of cytosolic Ca2+ we adapted a previously described method4-11 by omitting EGTA from the storage solution.
Already in 1970 it was observed that although myocytes dissociate in the presence of Ca2+ during digestion, all of them were in contracture and non-viable.16,17 Therefore, cell isolation is performed in Ca2+-free solution. However, the re-introduction of physiological concentrations of Ca2+ resulted in rapid Ca2+ influx and cell death. This has been described as the Ca2+ paradox phenomenon which was originally observed in perfused hearts by Zimmerman and Hulsman.18 Modifications of the isolation media including reduction of the pH to 7.0,19 addition of taurin20 or of small amounts of Ca2+ (see step 3.2 and 4.1),21 as well as storage of isolated myocytes in EGTA containing storage-solution22 have been suggested to prevent the Ca2+ paradox.17 However, it is well known that Ca2+ buffering through EGTA reduces the amplitude of L-type Ca2+ current-induced Ca2+ transient amplitudes and results in a biphasic decay of the Ca2+ transients.23 Therefore, we omitted EGTA throughout the whole isolation process in order to obtain Ca2+ transients with typical properties and monophasic decays. To protect the cells from the Ca2+ paradox we increased the final Ca2+ concentration of the storage solution in a stepwise manner until 0.2 mM.
The choice of collagenase is probably the most critical step for successful myocyte isolation. Conventional collagenases are crude preparations obtained from Clostridium histolyticum and contain collagenase in addition to a number of other proteinases, polysaccharidases and lipases. Based on their general composition collagenases are subdivided into different types.24 Worthington collagenase Types I and II have been successfully used for isolation of human atrial myocytes.4-10,15,25-30 In our presently described protocol we recommend the use of collagenase Type I, although we were also able to obtain acceptable amounts of viable cells using collagenase Type II. However, even within a single collagenase type there is a significant batch-to-batch variation regarding the enzyme activities. These variations require careful batch selection and testing of various batches to optimize isolation procedure. The online available batch-selection tool from Worthington Biochemical Corp. (<a href="http://www.worthington-biochem.com/cls/match.php" target="_blank">http://www.worthington-biochem.com/cls/match.php</a>) may be used to find available batches with a composition that has been shown to be suitable for the isolation of human atrial myocytes. Currently we use collagenase type I with 250 U/mg collagenase activity, 345 U/mg caseinase activity, 2.16 U/mg clostripain activity and 0.48 U/mg tryptic activity (lot# 49H11338).
 
 
The cells obtained using the procedure described in this manuscript may be used within 8 hr for patch-clamp studies, Ca2+ transient measurements and a combination of both.15 In addition, these cells allow measurements of cellular contraction in response to electric field stimulation or electric stimulation using the patch-clamp pipette (unpublished observations).

Studying electrophysiological properties of cardiac ion channels with the patch-clamp technique and the exploration of cellular Ca2+ handling abnormalities require isolated cardiomyocytes. These are usually obtained following the in vitro exposure of cardiac tissue samples to digestive enzymes (collagenase, hyaluronidase, peptidase etc.). Since the first report of isolation of viable cardiac myocytes in 19552 a large quantity of protocols has been developed in order to harvest single atrial and ventricular cardiomyocytes from different species including mouse, rat, rabbit, dog, guinea pig and human. In this review we focus on isolation of human atrial myocytes. Regarding procedures for isolation of myocytes from other species we refer to the "Worthington Tissue Dissociation guide" provided by Worthington Biochemical Corp., USA (<a href="http://www.tissuedissociation.com" target="_blank">www.tissuedissociation.com</a>).
Human atrial myocyte isolation protocols are generally derived from the method described by Bustamante, et al.3 Here we provide a step-by-step description of a technique, which is adapted from a previously published method, in order to obtain atrial myocytes suitable not only for patch-clamp experiments but also for simultaneous intracellular Ca2+ measurements.4-11

<table><tbody><tr><td> </td><td></td><td></td><td>&lt;em&gt;Transport solution&lt;/em&gt;</td></tr><tr><td>Albumin</td><td>Sigma-Aldrich</td><td>A3059</td><td>&lt;em&gt;Storage solution&lt;/em&gt;: 1%</td></tr><tr><td>BDM</td><td>Sigma-Aldrich</td><td>31550</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 30</td></tr><tr><td>DL-b-Hydroxy-butyric acid</td><td>Sigma-Aldrich</td><td>H6501</td><td>&lt;em&gt;Storage solution&lt;/em&gt;: 10</td></tr><tr><td>Glucose</td><td>Sigma-Aldrich</td><td>G8270</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 20&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 20&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 20&lt;br/&gt; &lt;em&gt;Storage solution&lt;/em&gt;: 10</td></tr><tr><td>L-Glutamic acid</td><td>Sigma-Aldrich</td><td>G1251</td><td>&lt;em&gt;Storage solution&lt;/em&gt;: 70</td></tr><tr><td>KCl</td><td>Merck</td><td>1049360250</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 10&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 10&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 10&lt;br/&gt; &lt;em&gt;Storage solution&lt;/em&gt;: 20</td></tr><tr><td>KH2PO4</td><td>Sigma-Aldrich</td><td>P5655</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 1.2&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 1.2&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 1.2&lt;br/&gt; &lt;em&gt;Storage solution&lt;/em&gt;: 10</td></tr><tr><td>MgSO4</td><td>Sigma-Aldrich</td><td>M9397</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 5&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 5&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 5</td></tr><tr><td>MOPS</td><td>Sigma-Aldrich</td><td>M1254</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 5&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 5&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 5</td></tr><tr><td>NaCl</td><td>Sigma-Aldrich</td><td>S3014</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 100&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 100&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 100</td></tr><tr><td>Taurin</td><td>Sigma-Aldrich</td><td>86330</td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 50&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 50&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 50&lt;br/&gt; &lt;em&gt;Storage solution&lt;/em&gt;: 10</td></tr><tr><td>Collagenase I</td><td><a href="http://www.worthington-biochem.com/" target="_blank"><img src="/img/new_window.png"> Worthington</a></td><td>4196</td><td>&lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 286 U/ml</td></tr><tr><td>Protease XXIV</td><td>Sigma-Aldrich</td><td>P8038</td><td>&lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 5 U/ml*</td></tr><tr><td>pH</td><td></td><td></td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 7.00&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 7.00&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 7.00&lt;br/&gt; &lt;em&gt;Storage solution&lt;/em&gt;: 7.40</td></tr><tr><td>adjusted with</td><td></td><td></td><td>&lt;em&gt;Transport solution&lt;/em&gt;: 1 M NaOH&lt;br/&gt; &lt;em&gt;Ca2+-free solution&lt;/em&gt;: 1 M NaOH&lt;br/&gt; &lt;em&gt;Enzyme solution E1 and E2&lt;/em&gt;: 1 M NaOH&lt;br/&gt; &lt;em&gt;Storage solution&lt;/em&gt;: 1 M KOH</td></tr><tr><td colspan="4">Concentrations in mM unless otherwise stated. BDM, 2,3-Butanedione monoxime. *Protease XXIV is included in Enzyme solution E1 only.</td></tr><tr><td colspan="4">&lt;strong&gt;Table I. Solutions.&lt;/strong&gt;</td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td>Nylon mesh (200 &amp;#956;m)</td><td>VWR-Germany</td><td>510-9527</td><td></td></tr><tr><td>Jacketed reaction beaker</td><td>VWR</td><td>KT317000-0050</td><td></td></tr><tr><td colspan="4">&lt;strong&gt;Table II. Specific equipment.&lt;/strong&gt;</td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td>Dimethyl-sulphoxide</td><td>Sigma-Aldrich</td><td>D2650</td><td></td></tr><tr><td>Fluo-3 AM (special packaging)</td><td>Invitrogen</td><td>F-1242</td><td></td></tr><tr><td>Pluronic F-127</td><td>Invitrogen</td><td>P6867</td><td></td></tr><tr><td colspan="4">&lt;strong&gt;Table III. Substances for loading of myocytes with Fluo-3 AM.&lt;/strong&gt;</td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td>4-aminopyridine*</td><td>Sigma-Aldrich</td><td>A78403</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 5</td></tr><tr><td>BaCl2*</td><td>Sigma-Aldrich</td><td>342920</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 0.1</td></tr><tr><td>CaCl2 &amp;#215; 2H2O</td><td>Sigma-Aldrich</td><td>C5080</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 2</td></tr><tr><td>Glucose</td><td>Sigma-Aldrich</td><td>G8270</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 10</td></tr><tr><td>HEPES</td><td>Sigma-Aldrich</td><td>H9136</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 10</td></tr><tr><td>KCl</td><td>Merck</td><td>1049360250</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 4</td></tr><tr><td>MgCl &amp;#215; 6H2O</td><td>Sigma-Aldrich</td><td>M0250</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 1</td></tr><tr><td>NaCl</td><td>Sigma-Aldrich</td><td>S3014</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 140</td></tr><tr><td>Probenecid</td><td>Sigma-Aldrich</td><td>P8761</td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 2</td></tr><tr><td>pH</td><td></td><td></td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 7.35</td></tr><tr><td>adjusted with</td><td></td><td></td><td>&lt;em&gt;Bath solution&lt;/em&gt;: 1 M HCl</td></tr><tr><td colspan="4">&lt;strong&gt;Table IV. Bath solution for patch-clamp.&lt;/strong&gt; *4-aminopyridine and BaCl were included for voltage-clamp experiments only.</td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td>DL-aspartat K+-salt</td><td>Sigma-Aldrich</td><td>A2025</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 92</td></tr><tr><td>EGTA</td><td>Sigma-Aldrich</td><td>E4378</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 0.02</td></tr><tr><td>GTP-Tris</td><td>Sigma-Aldrich</td><td>G9002</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 0.1</td></tr><tr><td>HEPES</td><td>Sigma-Aldrich</td><td>H9136</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 10</td></tr><tr><td>KCl</td><td>Merck</td><td>1049360250</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 48</td></tr><tr><td>MgATP</td><td>Sigma-Aldrich</td><td>A9187</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 1</td></tr><tr><td>Na2ATP</td><td>Sigma-Aldrich</td><td>A2383</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 4</td></tr><tr><td>Fluo-3**</td><td>Invitrogen</td><td>F3715</td><td>&lt;em&gt;Pipette solution&lt;/em&gt;: 0.1</td></tr><tr><td>pH</td><td></td><td></td><td>7.20</td></tr><tr><td>adjusted with</td><td></td><td></td><td>1 M KOH</td></tr><tr><td colspan="4">&lt;strong&gt;Table V. Pipette solution for patch-clamp*. &lt;/strong&gt;*On experimental days pipette solution is stored on ice until use. **Fluo-3 is added from a 1 mM stock solution on experimental days.</td></tr><tr><td></td><td></td><td></td><td></td></tr><tr><td></td><td></td><td></td><td></td></tr></tbody></table>

isolation of human atrial myocytes for simultaneous measurements of ca2+ transients and membrane currents

Isolation of Human Atrial Myocytes for Simultaneous Measurements of Ca2+ Transients and Membrane Currents

The study of electrophysiological properties of cardiac ion channels with the patch-clamp technique and the exploration of cardiac cellular Ca2+ handling abnormalities requires isolated cardiomyocytes. In addition, the possibility to investigate myocytes from patients using these techniques is an invaluable requirement to elucidate the molecular basis of cardiac diseases such as atrial fibrillation (AF).1 Here we describe a method for isolation of human atrial myocytes which are suitable for both patch-clamp studies and simultaneous measurements of intracellular Ca2+ concentrations. First, right atrial appendages obtained from patients undergoing open heart surgery are chopped into small tissue chunks ("chunk method") and washed in Ca2+-free solution. Then the tissue chunks are digested in collagenase and protease containing solutions with 20 &mu;M Ca2+. Thereafter, the isolated myocytes are harvested by filtration and centrifugation of the tissue suspension. Finally, the Ca2+ concentration in the cell storage solution is adjusted stepwise to 0.2 mM. We briefly discuss the meaning of Ca2+ and Ca2+ buffering during the isolation process and also provide representative recordings of action potentials and membrane currents, both together with simultaneous Ca2+ transient measurements, performed in these isolated myocytes.

Figure 2A shows three representative examples from isolated human right atrial myocytes. To quantify the cell yield we pipette 10 μl of cell suspension (step 5.5) on a CellFinder microscope slide (<a href="http://www.antenna.nl/microlab/index-uk.html" target="_blank">http://www.antenna.nl/microlab/index-uk.html</a>). Averaged cell yields in Figure 2B clearly indicate that there is a tendency to lower cell yields in chronic AF (cAF) patient samples (tube A: 16.5±3.1 cells/10 μl (n=29) vs. 5.1±2.3 cells/10 μl (n=10) in SR and cAF, respectively, p&lt;0.05; tube B: 17.9±3.9 cells/10 μl (n=29) vs. 5.9±2.0 cells/10 μl (n=9) in SR and cAF, respectively, p=0.107).
Representative examples of action-potential measurements and simultaneous recordings of cytosolic Ca2+ transients are given in Figure 3. In about 90% of the investigated cells, the action-potential-triggered Ca2+ release causes clear and regular cell contractions. As reported previously, the resting membrane potential, which is an accepted indicator for cell integrity, averaged about -73.9±2.7 mV (n = 23/10 myocytes/patients) and -77.7±1.8 mV (n = 19/8 myocytes/patients) in SR and cAF respectively (p&gt;0.05).15 Figure 4 shows representative simultaneous recordings of voltage-gated L-type Ca2+ currents and cytosolic Ca2+ transients. Application of the non-selective β-adrenoceptor agonist isoprenaline (1 μM) increases amplitudes of both ICa,L and cytosolic Ca2+ transients, suggesting intact β-adrenergic signal transduction cascade.
<img alt="Protocol diagram for loading human atrial myocytes with Fluo-3 AM; steps include cell suspension." fo:content-width="4in" fo:src="/files/ftp_upload/50235/50235fig1highres.jpg" src="/files/ftp_upload/50235/50235fig1.jpg" data-altupdatedat="1787630408000" data-alt="Figure 1"> 
Figure 1. Flow chart of the myocytes Fluo-3 AM loading protocol (see step 6.1-6.5). m/v, mass/volume.
<img alt="Microscopy and bar graph of cell yield in sinus rhythm vs. atrial fibrillation, highlighting trituration effect." fo:content-width="4in" fo:src="/files/ftp_upload/50235/50235fig2highres.jpg" src="/files/ftp_upload/50235/50235fig2.jpg" data-altupdatedat="1787630408000" data-alt="Figure 2"> 
Figure 2. A, Isolated human right atrial myocytes after one hour in storage solution. B, Mean±SEM of the cell yield counted in 10 μl of cells in storage solution (see step 5.5). n refers to the number of preparations within each group. *p&lt;0.05.
<img alt="Sinus rhythm vs atrial fibrillation chart; current, voltage, calcium levels over 200 ms interval." fo:content-width="4in" fo:src="/files/ftp_upload/50235/50235fig3highres.jpg" src="/files/ftp_upload/50235/50235fig3.jpg" data-altupdatedat="1787630408000" data-alt="Figure 3"> 
Figure 3. Representative recordings of action-potential-triggered Ca2+-transients (CaT) in an atrial myocyte from a sinus rhythm and a chronic atrial fibrillation patient. Top: Injected membrane current (IM) used for stimulation (0.5 Hz). Below: Simultaneous recording of membrane potential (VM), and triggered CaT (bottom). (Replotted with permission from Voigt et al. 2012)15
<img alt="Electrophysiology: Cardiac action potentials and calcium transients in sinus rhythm vs atrial fibrillation charts." fo:content-width="4in" fo:src="/files/ftp_upload/50235/50235fig4highres.jpg" src="/files/ftp_upload/50235/50235fig4.jpg" data-altupdatedat="1787630408000" data-alt="Figure 4"> 
Figure 4. Representative recordings of the isoprenaline (1 μM) effect on L-type Ca2+ current-triggered Ca2+-transients (CaT) in an atrial myocyte from a sinus rhythm and a chronic atrial fibrillation patient. Top: Voltage-clamp protocol (0.5 Hz). Below: Simultaneous recording of total net membrane current (IM), predominantly reflecting L-type Ca2+ current (middle) and triggered CaT (bottom). (Replotted with permission from Voigt, et al. 2012)15

<img src="/files/ftp_upload/50235/50235table1.jpg" alt="Chemical solutions preparation table; concentrations for cell transport and enzyme solutions." fo:content-width="4in" fo:src="/files/ftp_upload/50235/50235table1highres.jpg" data-altupdatedat="1787630408000" data-alt="Table 1"> 
Table I. Solutions. 
<img src="/files/ftp_upload/50235/50235table2.jpg" alt="Nylon mesh and jacketed beaker, VWR catalog, equipment list, 200 μm, laboratory setup." fo:content-width="2in" fo:src="/files/ftp_upload/50235/50235table2highres.jpg" data-altupdatedat="1787630408000" data-alt="Table 2"> 
Table II. Specific equipment. 
<img src="/files/ftp_upload/50235/50235table3.jpg" alt="Chemical reagents table with dimethyl-sulphoxide, Fluo-3 AM, Pluronic F-127 catalogue details." fo:content-width="2in" fo:src="/files/ftp_upload/50235/50235table3highres.jpg" data-altupdatedat="1787630408000" data-alt="Table 3"> 
Table III. Substances for loading of myocytes with Fluo-3 AM. 
<img src="/files/ftp_upload/50235/50235table4.jpg" alt="Chemical composition table for voltage-clamp experiments; includes reagents, concentrations, pH adjustment." fo:content-width="2.5in" fo:src="/files/ftp_upload/50235/50235table4highres.jpg" data-altupdatedat="1787630408000" data-alt="Table 4"> 
Table IV. Bath solution for patch-clamp. 
<img src="/files/ftp_upload/50235/50235table5.jpg" alt="Chemical reagent table, Sigma-Aldrich, Merck, Invitrogen, concentrations, pipette solution." fo:content-width="2.5in" fo:src="/files/ftp_upload/50235/50235table5highres.jpg" data-altupdatedat="1787630408000" data-alt="Table 5"> 
Table V. Pipette solution for patch-clamp*.

We describe the isolation of human atrial myocytes which can be used for intracellular Ca2+ measurements in combination with electrophysiological patch-clamp studies.

The study of  electrophysiological properties of cardiac ion channels with the patch-clamp  technique and the exploration of cardiac cellular Ca2+ ...

The overall goal of this procedure is to isolate human atrial myocytes suitable for simultaneous measurements of calcium, transients and membrane currents. The right atrial specimen is obtained from patients undergoing open heart surgery and is quickly transported to begin the procedure. The first step of the procedure is to clean the tissue and cut it into small tissue chunks.The second step is a twofold enzymatic digestion of the tissue with proteolytic enzymes resulting in isolated atrial myocytes. The final step comprises loading of the myocytes with a calcium sensitive fluorescent dye. Ultimately, the combined usage of epi fluorescence microscopy and the patch clamp technique produce simultaneous recordings of calcium transients with membrane currents or action potentials.This method can help to understand the molecular basis of cellular calcium handling abnormalities underlying cardiac diseases such as atrial fibrillation, demonstrating the method will be Claudia Lira, the senior technician of our laboratory, The human atrial tissue obtained from patients undergoing open heart surgery for coronary bypass grafting, or mitral valve replacement should be quickly transported to the lab in transport solution. Once at the lab, transfer the tissue sample and the solution to a 10 centimeter dish. Then roughly remove the fatty tissue using scissors.Next, wave the tissue sample. Keep between 200 and 600 milligrams for the cell isolation and freeze the remainder in liquid nitrogen for biochemical analysis. Transfer the tissue for cell isolation into a dish of cool calcium free solution and chop the tissue into one cubic millimeter chunks to wash the tissue.Transfer it together with the calcium free solution to the jacketed beaker. Heated to 37 degrees. Provide oxygen from a line capped with a pipette tip to prevent strong bubbling.Stir the tissue carefully for about three minutes with a magnetic stir bar. Then allow the tissue to settle. Now carefully strain the supernatant through a 200 micron nylon mesh.Most of the tissue should remain in the beaker. Refill the beaker with warmed 37 degree calcium free solution. Then return the strained tissue chunks from the mesh into the beaker using forceps and repeat the washing procedure twice.Begin this portion of the procedure by preparing 20 milliliters of warmed 37 degrees Celsius enzyme solution E one containing collagenase and protease. Carefully strain the calcium free solution after the final washing step and resuspend the washed tissue in the E one solution. Return the tissue collected on the mesh to the beaker.Stir the suspension carefully for 10 minutes. Then add 40 microliters of 10 millimolar calcium chloride, and continue stirring for 35 minutes. Next, strain the supernatant carefully through a nylon mesh.Most of the tissue should remain in the beaker. Prepare 20 milliliters enzyme solution E two containing collagenase one only, and use it to refill the beaker. Return the tissue collected on the mesh to the beaker.Then immediately add 40 microliters of 10 millimolar calcium chloride solution during the second digestion, occasionally use scissors to chop up tissue clots. After five minutes, take a sample of the suspension to check the dissociation of the cells under a microscope. Keep taking samples every two to three minutes until rod-shaped striated cardiomyocytes are clearly visible.Then stop the stirring, allowing the tissue to settle. Once settled, carefully strained the supernatant through a nylon mesh and into a plastic 50 milliliter tube. Next, suspend the tissue in 20 milliliters storage solution and return the strained tissue chunks from the mesh to the beaker.Further dissociate the cells by gentle mechanical tation. With a 20 milliliter pipette, try to avoid bubble formation. Next, carefully strain the supernatant through a nylon mesh after the straining centrifuge, both supernatant collections at 90 5G for 10 minutes.To pellet the cells, discard the supernatants by aspiration without disturbing the pellet resus. Suspend each pellet in 1.5 milliliters of storage solution at room temperature. Next, add 7.5 microliters of 10 millimolar calcium chloride solution to each tube and wait 10 minutes.Then add 7.5 more microliters of calcium chloride, and wait another 10 minutes. After the wait, add a third 15 microliter volume of 10 millimolar calcium chloride to bring the final concentration of calcium chloride in solution to 0.2 millimolar. The purpose of this isolation is to achieve cells which are suitable for intracellular calcium measurements.Therefore, it is a critical requirement to omit any calcium buffers such as EGGA from the storage solution. Transfer 1.5 milliliters of the cell suspension into a two milliliter micro centrifuge tube. The following steps should be executed under consideration of the light sensitivity of the fluorescent calcium indicator.Flu O three. First, make a one millimolar flu oh 3:00 AM stock solution. This solution can be stored at negative 20 degrees Celsius for up to one week.Next, add 15 microliters of the flu oh 3:00 AM stock solution to the 1.5 milliliter cell suspension. Agitate the mixture carefully and incubate the suspension for 10 minutes at room temperature in an opaque box. After the incubation, briefly centrifuge the tissue at about 6, 000 RPM.Then discard the supernatant and resuspend the pellet in 1.5 milliliters of bath solution. Leave the cell suspension for about 30 minutes for d esterification before beginning the experiments. Then proceed with simultaneous patch clamp and epi fluorescent calcium measurements using the outlined protocol.Myocytes were isolated from atrial tissue and quantified on a cell finder microscope slide. Average cell yields clearly indicate that there is a tendency to lower cell yields in samples from patients with chronic atrial fibrillation. Flu oh three loaded myocytes were stimulated at 0.5 hertz in current clamp configuration to elicit action potentials, about 90%of the investigated cells showed regular contractions.In response to this stimulation, the switch to fluorescence microscopy visualizes the action potential triggered calcium release from the sarcoplasmic reticulum, which initiates the cellular contraction. Representative recordings from patients with sinus rhythm and atrial fibrillation show that sr. Patient action potentials typically have a spike and dome shape, whereas action potential triangulation and shortening are typical hallmarks of atrial remodeling.In atrial fibrillation patients simultaneously recorded intracellular calcium transients revealed increased diastolic calcium levels and reduced calcium transient amplitude in myocytes from atrial fibrillation patients to record L type calcium currents. Potassium currents were blocked using four amino paridine and barium chloride. The cells were stimulated at 0.5 hertz in voltage clamp configuration using a holding potential of minus 80 millivolts with a 100 milliseconds ramp to minus 40 millivolts and a 100 millisecond test pulse to 10 millivolts.Representative recordings show that atrial fibrillation is associated with a reduced L type calcium current. Again, the diastolic calcium level was increased, whereas the calcium transient amplitude was lower. In atrial fibrillation.Application of the non-selective beta adrenal receptor agonist isoprene increased the amplitudes of L type calcium currents and cytosolic calcium transient. In both groups, this suggests the cells have an intact beta adrenergic signal transduction cascade. The results show that this method provides high quality calcium tolerant myocytes, which are suitable for simultaneous patch clamp and calcium transient measurements.In addition, the obtained myocytes may be useful for cell shortening measurements, immune staining, or TTU staining.

isolation-human-atrial-myocytes-for-simultaneous-measurements-ca2

Research

JoVE Journal

Biology

Kv channel dysfunction is associated with cardiac arrhythmias. In order to study the molecular mechanisms that lead to such arrhythmias we utilize a systematic protocol for isolation of atrial and ventricular cardiomyocytes from Kv channel ancillary subunit knockout mice. Isolated cardiomyocytes can then immediately be used for cellular electrophysiological studies, biochemical or immunofluorescence (IF) assays.

Isolation and Kv Channel Recordings in Murine Atrial and Ventricular Cardiomyocytes

Current knowledge on the cellular basis of cardiac diseases mostly relies on studies on animal models. Here we describe and validate a novel method to obtain single viable cardiomyocytes from small surgical samples of human ventricular myocardium. Human ventricular myocytes can be used for electrophysiological studies and drug testing.

Isolation and Functional Characterization of Human Ventricular Cardiomyocytes from Fresh Surgical Samples

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.

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

This protocol describes the electrophysiological evaluation of murine atria utilizing an optical mapping system with a high temporal and spatial resolution, including dual recordings of the membrane voltage and Ca2+ transient under programmed stimulation through a specialized electrode catheter.

Electrophysiological Assessment of Murine Atria with High-Resolution Optical Mapping

Here, we describe an optimized, Langendorff-based procedure for the isolation of single-cell atrial cardiomyocytes from a rat model of metabolic syndrome-related heart failure with preserved ejection fraction. A manual regulation of intraluminal pressure of cardiac cavities is implemented to yield functionally intact myocytes suitable for excitation-contraction-coupling studies.

Isolation of Atrial Cardiomyocytes from a Rat Model of Metabolic Syndrome-related Heart Failure with Preserved Ejection Fraction

This protocol is used to isolate single atrial cardiomyocytes from the adult mouse heart using a chunk digestion approach. This approach is used to isolate right or left atrial myocytes that can be used to characterize atrial myocyte electrophysiology in patch-clamp studies.

Isolation of Atrial Myocytes from Adult Mice

Presented is a protocol for the isolation of human and animal ventricular cardiomyocytes from vibratome-cut myocardial slices. High yields of calcium-tolerant cells (up to 200 cells/mg) can be obtained from small amounts of tissue (&lt;50 mg). The protocol is applicable to myocardium exposed to cold ischemia for up to 36 h.

Isolation of Human Ventricular Cardiomyocytes from Vibratome-Cut Myocardial Slices

A method is described for the simultaneous isolation of myocytes and non-myocytes from both the atria and ventricles of a single adult mouse heart. This protocol results in consistent yields of highly viable cardiac myocytes and non-myocytes and details optimal cell-specific culture conditions for phenotyping and in vitro analysis.

Simultaneous Isolation and Culture of Atrial Myocytes, Ventricular Myocytes, and Non-Myocytes from an Adult Mouse Heart

Mouse models allow studying key mechanisms of arrhythmogenesis. For this purpose, high quality cardiomyocytes are necessary to perform patch-clamp measurements. Here, a method to isolate murine atrial and ventricular myocytes via retrograde enzyme-based Langendorff perfusion, which allows simultaneous measurements of calcium-transients and L-type calcium current, is described.

Isolation of High Quality Murine Atrial and Ventricular Myocytes for Simultaneous Measurements of Ca2+ Transients and L-Type Calcium Current

This protocol describes modifications of the Langendorff method including the depth of aorta cannulation for simultaneous Isolation of atrial and ventricular myocytes from adult mice.

Modifications of the Langendorff Method for Simultaneous Isolation of Atrial and Ventricular Myocytes from Adult Mice

Learn to isolate human atrial myocytes for simultaneous measurements of calcium transients and membrane currents using enzymatic digestion and patch clamp techniques. This method advances cardiac disease research.

Isolation of Human Atrial Myocytes for Simultaneous Measurements of Ca²⁺ Transients and Membrane Currents

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