E.A.B. was supported by the National Institutes of Health (1F31HL140850), the ARCS Foundation, Inc., San Diego Chapter, and is a Rees-Stealy Research Foundation Phillips Gausewitz, M.D. Scholar of the SDSU Heart Institute. E.A.B. and A.S.B. were supported by the Inamori Foundation. CCG by (NIH) grants R01 HL135893, R01 HL141463 and HL149931.

All research performed on mice reported in this paper has been reviewed and approved by the SDSU Institutional Animal Care and Use Committee and it conforms to the Guide for the Care and Use of Laboratory Animals published by the National Research Council.
1. Preparation of isolation and culture media and plating
<ol>
	<li>Prepare 1 L of heart perfusion media prior to use by adding Joklik modified minimum essential media (MMEM) to 1 L of sterile water. Adjust the pH to 7.36 with 10 N NaOH, then filter through a 0.2 &#181;m filter and store at 4 &#176;C for up to 2 weeks. 
	NOTE: Joklik MMEM consists of 112 mM NaCl, 5.4 mM KCl, 1 mM MgCl2, 9 mM NaH2PO4, and 11.1 mM D-glucose. This is supplemented with 10 mM HEPES (2.38 g/L), 30 mM taurin (3.75 g/L), 2 mM D-l-carnitine (0.4 g/L), 2 mM creatine, and 10 mM butanedione monoxime (1.01 g/L).</li>
	<li>Prepare digestion buffer just prior to perfusion, as follows: supplement 50 mL of heart perfusion media with 6.25 &#181;L of 100 mM CaCl2 (see step 1.3) and collagenase type 2 (enzymatic activity ~310&#8211;320 U/mg dw). 
	NOTE: Weigh the animal prior to sacrifice. The amount of collagenase type 2 supplemented into the digestion buffer is dictated by the weight of the animal (2.25 mg of collagenase type 2 per 1 g of body weight).</li>
	<li>To prepare 100 mM CaCl2, add 1.47 g of CaCl2 to 100 mL of molecular biology grade water. Stir until dissolved, then pass through a 0.2 &#181;m filter and store at room temperature for up to 2 months.</li>
	<li>Prepare myocyte stopping buffer 1 by supplementing 90 mL of heart perfusion buffer with 10 mL of fetal bovine serum (FBS) and 125 &#181;L of 100 mM CaCl2. Pass through a 0.2 &#181;m filter and store at 4 &#176;C for up to 2 weeks.</li>
	<li>Prepare myocyte stopping buffer 2 by supplementing 114 mL of heart perfusion buffer with 6 mL of FBS and 150 &#181;L of 10 mM CaCl2. Pass through a 0.2 &#181;m filter and store at 4 &#176;C for up to 2 weeks.</li>
	<li>Prepare atrial myocyte plating medium just prior to perfusion by supplementing 95 mL of Dulbecco&#8217;s modified Eagle medium (DMEM) with 4 mL of FBS, 1 mL of 100x pen/strep-glutamine, 1 mL of 100x insulin-transferrin-selenium, and 1 mL of 10 &#181;M dexamethasone. Pass through a 0.2 &#181;m filter and store at 37 &#176;C until plating.</li>
	<li>Prepare ventricular myocyte plating medium by supplementing 95 mL of minimum essential medium (MEM) with 4 mL of FBS, 1 mL of 100x pen/strep-glutamine, 10 mL of 1 M HEPES solution, 1 mL of 100x insulin-transferrin-selenium, and 0.1 g of butanedione monoxime. Pass through a 0.2 &#181;m filter and store at 4 &#176;C for up to 2 weeks.</li>
	<li>Prepare ventricular myocyte maintaining medium by supplementing 99 mL of MEM with 1 mL of 100x insulin-transferrin-selenium, 0.1 mg/mL bovine serum albumin (BSA), 10 mL of 1 M HEPES solution and 1 mL of 100x pen/strep-glutamine. Pass through a 0.2 &#181;m filter and store at 4 &#176;C for up to 2 weeks.</li>
	<li>To prepare laminin-coated experimental plates and slides, thaw mouse laminin stock solution (1.19 mg/mL). Add 10 &#181;L of laminin stock solution to every 1 mL of DMEM, and mix. Coat experimental plates and slides evenly and store in a 37 &#176;C, 5% CO2 incubator for at least 1 h prior to perfusion to allow for equilibration. 
	NOTE: Coated experimental plates and slides can be stored at 4 &#176;C for up to 2 days.</li>
</ol>
2. Isolation apparatus
<ol>
	<li>Prior to each isolation, clean the tubing and other components of the system with three complete washes of 70% EtOH by filling the bubble trap to the top (close off the bottom stopcock and keep the top stopcock open).</li>
	<li>Rinse the complete system 3x with sterile H2O by filling the bubble trap to the top (close off the bottom stopcock and keep the top stopcock open).</li>
	<li>Rinse out the complete system with heart perfusion buffer and fill the bubble trap halfway with media.</li>
	<li>Set the circulating water bath to 37 &#176;C.</li>
	<li>Set a water bath for media to 37 &#176;C.</li>
	<li>Remove any air bubbles in the peristaltic pump tubing.</li>
	<li>Adjust the flow rate of the peristaltic pump to 3 mL/min.</li>
</ol>
3. Surgical procedure (non-survival)
<ol>
	<li>Soak surgical instruments in 70% EtOH for at least 5 min.</li>
	<li>Place the heart perfusion media, myocyte stopping buffers, and digestion buffer in the 37 &#176;C water bath.</li>
	<li>Place the atrial myocyte plating medium, ventricular myocyte plating medium, and ventricular myocyte maintaining medium in a 37 &#176;C, 5% CO2 incubator 1 h prior to use and loosen the caps to allow equilibration.</li>
	<li>Inject 10-week-old male or female C57b6/j mice intraperitoneally (i.p.) with 0.35 mL of heparin, diluted in phosphate buffered saline (PBS) to 100 IU/mL. Allow the drug to take effect for about 10 min. 
	NOTE: If two hearts are to be subjected to this isolation procedure, the second mouse can be anesthetized and administered heparin at this point in the first procedure. To minimize stress on the animal, light anesthesia can be administered using 2% isoflurane/oxygen mixture in a hermetically sealed induction chamber.</li>
	<li>Anesthetize the animal with a 2% isoflurane/oxygen mixture and inject i.p. with pentobarbital (0.3 mL from 10 mg/mL stock), then prepare the chest by swabbing with 70% EtOH.</li>
	<li>Prepare a tied 5-0 silk suture to be ready to ligate the heart to the perfusion cannula. Mount cannula right next to surgical microscope.</li>
	<li>Quickly open the chest by first making a midline skin incision, from mid-abdomen to the jaw, then entering the peritoneum with the large scissors, clearing the diaphragm away by blunt dissection. Then, cut away the rib cage using the scissors with cuts up the chest wall on the lateral aspect of both sides.</li>
	<li>Snip away fibrous connections between the heart and chest wall (including thymus). Then, cut away the rib cage all together. Using the small forceps and scissors, gently lift the heart by the apex and expose the posterior aspect of the heart.</li>
	<li>Explant the heart by dissecting immediately inferior to the innominate artery on the ascending aorta and immediately place the heart in ice-cold PBS or cold heart perfusion media. Subsequently, quickly dissect away remaining tissue from the explanted heart in ice-cold heart perfusion media, exposing the ascending aorta. 
	NOTE: It is useful to explant the heart with the thymus intact to use as an anatomical landmark.</li>
	<li>Clean the area surrounding the aorta of excess tissue using micro-dissecting forceps and scissors. Position the aorta onto the cannula using fine-tipped forceps and secure with a 5-0 silk suture. 
	NOTE: The best placement usually occurs with the aorta extending about 2 mm up on the cannula.</li>
	<li>Perfuse the cannulated heart with heart perfusion media at a flow rate of 3 mL/min for 4 min. Then switch the media from heart perfusion media to digestion buffer for 15.0&#8722;17.5 min of perfusion (Figure 1A). 
	NOTE: Coronary flow rate will likely increase, indicating effective tissue digestion (i.e., pale, swollen heart).</li>
	<li>Collect 8 mL of digestion buffer flow through during the final minutes of perfusion for later use in step 5.4.</li>
	<li>Remove the heart from the cannula and place it on a 60 mm plastic culture dish. Remove excess tissue (i.e., aorta, veins) and submerge the heart in 2.5 mL of digestion buffer in preparation for mechanical separation. 
	NOTE: At this point, the atria are dissected away, and one experimenter should conduct the atrial cell isolation protocol, while a second experimenter should conduct the ventricular cell isolation.</li>
</ol>
4. Atrial cell isolation and culture
<ol>
	<li>Dissect the atria away from the heart and place it into a 30 mm plastic culture dish. Submerge it in 0.75 mL of digestion buffer for mechanical separation. Keep the ventricles in the 60 mm dish (step 3.12) and carry out the separate isolation methods simultaneously (section 5, Figure 1B). 
	NOTE: At this point, the atria and ventricles can undergo further separation should there be a need to isolate the left- and right-side cells.</li>
	<li>Begin to mince and tease the atria apart, initially with fine-tip surgical scissors and followed by fine forceps for further mincing. Avoid agitating the tissue, and do not rapidly pull apart muscle fibers.</li>
	<li>Using a sterile transfer pipette tip, continue to gently mix and dissociate the tissue for 15 min. Every 5 min, observe atrial myocyte disassociation from tissue under a 10x objective brightfield microscope. As tissue becomes further digested, continue gently mixing and dissociating tissue using a sterile transfer pipette tip with a smaller pore size.</li>
	<li>Transfer cell suspension to a 2 mL sterile micro-centrifuge tube. Rinse the 30 mm plate with 0.75 mL of 37 &#176;C myocyte stopping buffer 1 and combine with the cell suspension (end volume = 1.5 mL).</li>
	<li>Allow the atrial myocytes to sediment by gravity for 10 min at room temperature. Gently agitate the cell suspension to allow for myocytes to sediment to the bottom of the conical tube, forming a visible pellet.</li>
	<li>Centrifuge the cell suspension for 5 min at 20 x g. Carefully remove the supernatant, which contains the non-myocytes, and transfer to a 15 mL polypropylene conical tube using a sterile pipette tip without disturbing the pellet of atrial myocytes.</li>
	<li>Centrifuge the non-myocyte fraction for 5 min at 20,000 x g. Aspirate the supernatant and resuspend the non-myocyte pellet in 10 mL of DMEM supplemented with 10% fetal calf serum (FCS).</li>
	<li>Count non-myocytes using a hemocytometer or other method, then plate as per experimental needs, or further isolate into individual specific cell populations via fluorescence-activated cell sorting (Figure 1C).</li>
	<li>Resuspend the pellet of isolated atrial myocytes from step 4.6 in 1 mL of atrial myocyte plating medium and apply 10 &#181;L of this suspension onto a hemocytometer. Perform a cell count of rod-shaped myocytes per field.</li>
	<li>Aspirate laminin from precoated experimental plates/slides and resuspend the isolated atrial myocytes in the appropriate volume of atrial myocyte plating medium supplemented with 25 &#181;M blebbistatin. Plate at the desired density per experimental needs (Figure 1C). 
	NOTE: Typical plating density for the long-term culturing described here is 5 x 105 cells/chamber on four-chamber (1.7 cm2) glass slides.</li>
</ol>
5. Ventricular cell isolation and culture
<ol>
	<li>Begin to mince and tease heart apart ventricular tissue, first with fine-tip surgical scissors and followed by fine forceps for further mincing (Figure 1B). Avoid agitating the tissue by rapidly pulling apart muscle fibers.</li>
	<li>Transfer the cell suspension to a 15 mL polypropylene conical tube. Rinse the plate with 2.5 mL of 37 &#176;C myocyte stopping buffer 1 and combine with the cell suspension (end volume = 5 mL).</li>
	<li>Using a sterile transfer pipette tip, continue to gently mix and dissociate the tissue for 4 min. Apply 10 &#181;L of this cell suspension onto the slide and visualize the presence of rod-shaped myocytes to ensure the quality of isolation.</li>
	<li>Pass the cell suspension through a 100 &#181;m sterile nylon filter into a 50 mL polypropylene conical tube. Use 2 mL of digestion buffer collected in step 3.12 to wash any remaining cells off the sterile nylon filter.</li>
	<li>Allow the ventricular myocytes to sediment by gravity for 6 min at room temperature. Gently agitate the filtered cell suspension to allow for myocytes to sediment at the bottom of the conical, forming a visible pellet.</li>
	<li>Without disturbing the pellet of ventricular myocytes, carefully remove the supernatant (non-myocytes) and transfer to a 50 mL polypropylene conical tube using a sterile pipette tip. Centrifuge the non-myocyte fraction for 5 min at 20,000 x g. Aspirate the supernatant and resuspend the non-myocyte pellet in 10 mL of DMEM supplemented with 10% FCS.</li>
	<li>Count non-myocytes using a hemocytometer and resuspend in an appropriate volume of DMEM supplemented with 10% FCS. Then, plate according to experimental needs, or further isolate into individual specific cell populations via fluorescence-activated cell sorting (Figure 1C).</li>
	<li>Resuspend the isolated ventricular myocytes in 2 mL of myocyte stopping buffer 2 and apply 10 &#181;L of cell suspension onto hemocytometer. Perform a cell count of rod-shaped myocytes per field.</li>
	<li>Reintroduction of Ca2+ using a stepwise paradigm 
	NOTE: Calcium reintroduction steps are specific for ventricular myocytes and should not be performed for atrial myocytes, as this will result in cell death.
	<ol>
		<li>Add 50 &#181;L of 10 mM CaCl2 to the ventricular myocyte cell suspension. Mix well and incubate for 4 min at room temperature.</li>
		<li>Add an additional 50 &#181;L of 10 mM CaCl2 to the ventricular myocyte cell suspension. Mix well and incubate for 4 min at room temperature.</li>
		<li>Add an additional 100 &#181;L of 10 mM CaCl2 to the ventricular myocyte cell suspension. Mix well and incubate for 4 min at room temperature.</li>
		<li>Add 80 &#181;L of 100 mM CaCl2 to the ventricular myocyte cell suspension. Mix well and incubate for 4 min at room temperature.</li>
	</ol>
	</li>
	<li>Remove laminin coating from plates or slides and resuspend the isolated ventricular myocytes in an appropriate volume of ventricular myocyte plating medium according to experimental needs (Figure 1C). 
	NOTE: Typical plating density for the long-term culturing described here is 5 x 105 cells/chamber on four-chamber (1.7 cm2) glass slides. Avoid plating at a density of greater than 75% confluency, as cellular over-densification promotes cell clumping, thereby inhibiting attachment to the plate. Furthermore, large numbers of cells will be lost during the first medium change. Plate cells quickly after isolation, as extracellular Ca2+ promotes hypercontraction and loss of viable myocytes.</li>
	<li>Allow the ventricular myocytes to settle and adhere for at least 1 h. Subsequently change the media to ventricular myocyte maintaining medium supplemented with 25 &#181;M blebbistatin. 
	NOTE: Ventricular myocytes can be cultured up to 96 h after plating in &#181;M blebbistatin. Experiments should be conducted in ventricular myocyte maintaining medium in the absence of blebbistatin.</li>
</ol>

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The authors have nothing to disclose.

The quality of the cells isolated using the procedure described here, as determined by the cell yield and overall health of the cells in culture, depends on numerous controllable factors. Starting with the mouse itself, it has been documented that stress imposed on the animal can negatively affect cell yield and viability in culture, presumably due to excess systemic cortisol, catecholamines, and the hypercontractile state of cardiac tissue2,5,7. For these reasons, measures should be taken to avoid alarming the animal prior to sacrifice. Such measures include covering the animal&#8217;s cage and limiting time outside of vivarium prior to sacrifice. Heparin and many barbiturates commonly used for euthanasia can affect signaling pathways; thus, the optimal method of euthanasia should be customized accordingly. The age of the animal has a considerable impact on the quality and viability of isolated cells, most likely due to progressive accumulation of interstitial fibrosis occurring concurrently with the aging process, which can affect tissue digestion25. In data not presented here, while the method described above works in mice of up to 78 weeks old, the quality of the cells was lower in these older animals.
The most critical step in the isolation process described, as well as other protocols featuring a Langendorff apparatus for retrograde perfusion, is the cannulation and initial perfusion of the heart. For optimum results, the time from cardiac explantation to cannulation of the ascending aorta and initiation of perfusion should take no more than 90 s. In addition to time, two additional important factors are the depth of cannula and possibility of introducing air emboli from the perfusion apparatus. Accordingly, the cannula should be advanced into the ascending aorta so as not to enter the aortic root and obstruct the aortic valve, which would impair perfusion of the coronary vessels.
During the digestion process, it is important to regularly test the rigidity of the heart to avoid prolonged exposure to the digestive enzyme collagenase, which reduces cardiac myocyte calcium tolerance. The protocol described above for calcium reintroduction into the isolated ventricular myocyte cultures was designed to limit cardiac myocyte death via inappropriate calcium influx via store operated calcium channels. It should be noted that the stepwise calcium reintroduction should not be performed for isolated atrial myocyte cultures, as this will promote cell death during short- and long-term culture12. For further precaution, the perfusion and digestion buffers used here include the cardiac muscle contraction inhibitor butanedione monoxime (BDM) to avoid hypercontraction of isolated myocytes, as well as the calcium paradox, both of which impact myocyte viability26. However, the switch from BDM to blebbistatin should be noted, as it is the preferred anti-contractile agent in maintaining media for isolated cardiac myocytes. In data not shown, blebbistatin confers greater viability for long-term culture of isolated cardiac myocytes.
Immediately after isolation, it is important to consider the ramifications of long-term culture of cardiac cells, especially myocytes. The cardiac non-myocyte isolation and culturing protocol described here is based on common methods that take advantage of the different densities and adhesive properties of different cardiac cells. The benefit of non-myocytes is their high expansion potential in culture; thus, unlike cardiac myocytes, they are amenable to passaging for perpetuation. However, it is known that culturing conditions, including medium supplementation with FBS, can affect cardiac myocyte functionality27. The culture media described here were designed to optimize viability and limit functional derangements, especially for the isolated atrial myocytes. While no overt impaired contractile ability was observed in isolated cardiac myocytes after culture in the absence of blebbistatin supplementation, studies that focus on electrophysiology, contractility, and other single-cell in vivo-based molecular signaling should be performed soon after isolation, when the sarcomeric structure and molecular signature still mimics that of the intact heart.
A hallmark feature of the atrial myocyte is its ability to moonlight as an endocrine cell with immense secretory capacity, in addition to their contractile function. Under physiological conditions, atrial myocytes produce large quantities of ANP, which is stored in the endoplasmic reticulum and in large dense-core secretory granules poised for regulated exocytosis upon receiving a stimulus16,17. While many isolated atrial myocyte studies focus on their unique electrophysiological properties, this is the first study to design a culture media. This allows for long-term viability as well as promotion of the maintained functions of endocrine and contractile properties of atrial myocytes. This novel method for culturing, as well as simultaneous isolation of all cell types from atrial and ventricular chambers from a single mouse heart, will be useful and efficacious for studies on the physiological and pathophysiological properties of both atrial and ventricular myocytes.&#160;

Primary cell culture is an integral resource that offers a controlled environment for detailed mechanistic studies of cardiac myocyte function. Due to their more durable nature and ease of isolation, neonatal rat atrial and ventricular myocytes have been the common source of such cell cultures1. However, adult mouse atrial and ventricular myocytes (AMAMs and AMVMs) are highly desirable for in vitro studies, because their molecular and functional characteristics better mimic those of adult heart cells. Thus, they have become relevant for studies related to cardiac pathologies, most of which develop in adults2.
Furthermore, the availability and use of transgenic and disease mouse models expands the utility of isolated adult cardiac myocytes. Protocols for the isolation and culture of mouse AMVMs for short- and long-term studies have been described in numerous previous publications2,3,4,5,6,7,8,9,10,11. In comparison, few protocols have been described for the isolation of AMAMs. Furthermore, those that are described are primarily optimized for acute studies of freshly isolated cells, with no long-term culturing protocol described to date11,12,13. As such, AMAM isolation protocols were not designed to provide the utility and versatility of published protocols for the isolation and culture of AMVMs. Furthermore, while the pioneering studies for the isolation of AMAMs and AMVMs have proven resourceful, there are no protocols for optimal concurrent isolation and culture of both AMAMs and AMVMs, which results in efficient use of the whole heart for each preparation.
Until now, published AMAM and AMVM isolation protocols were not designed for simultaneous isolation of both cell types, because most studies on atrial and ventricular function have a chamber-specific focus. For instance, AMAMs are used predominantly to study atrial myocyte electrophysiology, partly because of the interest in atrial fibrillation (AF), the most common cardiac arrhythmia in the U.S. However, AF is not a disease that affects the atria in isolation, and it has been implicated as having a causative role in mild to severe left ventricular dysfunction14. Furthermore, electrocardiograms from patients with heart failure with preserved ejection fraction (HFpEF) have illustrated that left atrial size is one of the strongest predictors for susceptibility to heart failure15.
In addition to its role in electrophysiology and contractility, the atrium is also an endocrine organ, secreting cardiokines (i.e., atrial natriuretic peptide [ANP]) that homeostatically regulate blood pressure and volume16,17. Moreover, ANP (presumably from atrial myocytes) has a prominent protective and anti-hypertrophic role in ventricular myocytes16,17. While there is a strong implication of neurohormonal communication between atria and ventricles in various disease states, the mechanisms underlying this communication has not been fully explored. This point is further exemplified by the surge in research focusing on 1) the role of non-myocytes (specifically cardiac fibroblasts and immune cells) in the diseased heart and 2) how cardiac remodeling as a function of disease directly affects cardiac myocyte viability and global cardiac function18,19,20,21,22. Thus, studying cardiac cells from both atria and ventricles is a necessary approach to gain a more complete picture of their roles in cardiac pathophysiology.
The following protocol describes the simultaneous isolation of atrial and ventricular myocytes and non-myocytes from a single mouse heart under physiological and pathophysiological conditions. Additionally, this method is the first to describe optimal conditions necessary for maintaining cultures of atrial cardiac myocytes, as conditions for maintaining cultures of ventricular myocytes have already been published.

<table><tbody><tr><td>(-)-Blebbistatin</td><td>Sigma-Aldrich</td><td>B0560</td><td></td></tr><tr><td>1 Liter Water Jacketed Reservoir</td><td>Radnoti</td><td>120142-1</td><td></td></tr><tr><td>2,3-Butanedione monoxime</td><td>Sigma-Aldrich</td><td>B0753</td><td></td></tr><tr><td>5-0 Silk Suture Thread</td><td>Fine Science Tools</td><td>18020-50</td><td></td></tr><tr><td>Adenosine</td><td>Sigma-Aldrich</td><td>A9251</td><td></td></tr><tr><td>Bovine Serum Albumin</td><td>Sigma-Aldrich</td><td>A6003</td><td></td></tr><tr><td>Bubble Trap Compliance Chamber</td><td>Radnoti</td><td>130149</td><td></td></tr><tr><td>Calcium Chloride Anhydrous</td><td>Fisher Scientific</td><td>C614-500</td><td></td></tr><tr><td>Carnitine hydrochloride</td><td>Sigma-Aldrich</td><td>C9500</td><td></td></tr><tr><td>Collagenase type 2</td><td>Worthington Biochemical Corporation</td><td>LS004176</td><td></td></tr><tr><td>Creatine</td><td>Sigma-Aldrich</td><td>C0780</td><td></td></tr><tr><td>Dexamethasone</td><td>Sigma-Aldrich</td><td>D2915</td><td></td></tr><tr><td>DMEM/F12 (1:1; 1X)</td><td>Gibco</td><td>11330-032</td><td></td></tr><tr><td>Dumont #7 - Fine Forceps</td><td>Fine Science Tools</td><td>11274-20</td><td></td></tr><tr><td>Epifluorescent micropscpe</td><td>Olympus X70</td><td>IX70</td><td></td></tr><tr><td>Fetal Bovine Serum (Heat Inactivated)</td><td>Omega Scientific</td><td>FB-12</td><td>Lot# 206018</td></tr><tr><td>Fine Scissors - Sharp</td><td>Fine Science Tools</td><td>14060-09</td><td></td></tr><tr><td>Graefe Forceps</td><td>Fine Science Tools</td><td>11051-10</td><td></td></tr><tr><td>Headband Magnifiers</td><td>Fine Science Tools</td><td>28030-04</td><td></td></tr><tr><td>Hemacytometer (Bright-Line)</td><td>Hausser Scientific</td><td>1475</td><td></td></tr><tr><td>HEPES (1M)</td><td>Gibco</td><td>15630-080</td><td></td></tr><tr><td>Inosine</td><td>Sigma-Aldrich</td><td>I4125</td><td></td></tr><tr><td>Insulin-Transferrin-Selenium-X</td><td>Gibco</td><td>51500-056</td><td></td></tr><tr><td>Isotemp 105 Water Bath</td><td>Fisher Scientific</td><td>NC0858659</td><td></td></tr><tr><td>Isotemp 3006</td><td>Fisher Scientific</td><td>13-874-182</td><td></td></tr><tr><td>Joklik Modified Minimum Essential Media</td><td>Sigma-Aldrich</td><td>M-0518</td><td></td></tr><tr><td>Laminin (Natural, Mouse)</td><td>Gibco</td><td>1795024</td><td>Lot# 1735572</td></tr><tr><td>L-Glutamine</td><td>Sigma-Aldrich</td><td>G8540</td><td></td></tr><tr><td>Masterflex C/L Single-Channel Variable-Speed Compact Pump</td><td>Cole-Palmer</td><td>EW-77122-24</td><td></td></tr><tr><td>Minimum Essential Medium (MEM 1X)</td><td>Gibco</td><td>12350-039</td><td></td></tr><tr><td>Molecular Biology Grade Water</td><td>Corning</td><td>46-000-CM</td><td></td></tr><tr><td>Pen Strep Glutamine (100X)</td><td>Gibco</td><td>10378-016</td><td></td></tr><tr><td>Spring Scissors - 6mm Cutting Edge</td><td>Fine Science Tools</td><td>15020-15</td><td></td></tr><tr><td>Taurine</td><td>Sigma-Aldrich</td><td>T-8691</td><td></td></tr></tbody></table>

simultaneous isolation and culture of atrial myocytes, ventricular myocytes, and non-myocytes from an adult mouse heart

The isolation and culturing of cardiac myocytes from mice has been essential for furthering the understanding of cardiac physiology and pathophysiology. While isolating myocytes from neonatal mouse hearts is relatively straightforward, myocytes from the adult murine heart are preferred. This is because compared to neonatal cells, adult myocytes more accurately recapitulate cell function as it occurs in the adult heart in vivo. However, it is technically difficult to isolate adult mouse cardiac myocytes in the necessary quantities and viability, which contributes to an experimental impasse. Furthermore, published procedures are specific for the isolation of either atrial or ventricular myocytes at the expense of atrial and ventricular non-myocyte cells. Described here is a detailed method for isolating both atrial and ventricular cardiac myocytes, along with atrial and ventricular non-myocytes, simultaneously from a single mouse heart. Also provided are the details for optimal cell-specific culturing methods, which enhance cell viability and function. This protocol aims not only to expedite the process of adult murine cardiac cell isolation, but also to increase the yield and viability of cells for investigations of atrial and ventricular cardiac cells.

A wildtype 10-week-old C57b6/j mouse heart typically results in between 75,000&#8722;150,000 atrial myocytes and 1.0&#8722;1.5 x 106 ventricular myocytes, equating to an approximate yield of 30%&#8722;50% for atrial and ventricular myocytes18,19. During and immediately after isolations, viable cardiac myocytes should appear rod-shaped and non-contracting. A majority of isolated cardiac myocytes should adapt this morphology, which is an indication of effective perfusion. The rod-shape morphology can also be a predictor of viability. The protocol aims to enhance the yield and viability of myocytes and non-myocytes isolated from a diseased mouse heart. Furthermore, it has been tested in a model of pressure overload-induced heart failure (data not shown).
To confirm adequate and replicable isolation of myocytes and non-myocytes from atrial and ventricular tissue, cells were observed and photographed at various days in culture (Figure 2). Additionally, quantitative reverse-transcription polymerase chain reaction (qRT-PCR) was performed to measure the levels of transcripts that were cell type-specific. Cardiac muscle troponin T (Tnnt2) is a marker of cardiac myocytes and was robustly expressed in both atrial and ventricular cardiac myocyte cultures (Figure 3A). In contrast, atrial natriuretic peptide (Nppa, which is typically expressed exclusively in adult atrial cardiac myocytes under physiological conditions) and myosin light chain 2 (Myl2, which is a ventricular myocyte specific gene) were robustly and specifically expressed in atrial and ventricular cardiac myocyte cultures, respectively (Figure 3B,C).
Fibroblast markers, transcription factor 21 (Tcf21), platelet-derived growth factor receptor A (Pdgfra), and monocyte-derived cell marker cluster of differentiation 68 (Cd68) were exclusively expressed in non-myocyte cultures isolated from both atrial and ventricular chambers (Figure 3D&#8722;F). It is estimated that non-myocytes compromise ~65% of all heart cells and that a majority of these originate from a fibroblast or monocyte-derived lineage18,19,23,24. Thus, markers for these two lineages were chosen to be representative, given the interest in these cellular populations in studies of various models and etiologies of cardiac pathology.
Immunostaining of AMAMs and AMVMs for the t-tubule marker dihydropyridine (DHPR, which is a voltage-dependent (L)-type calcium channel) as well as the ryanodine receptor (RYR2) demonstrated intact t-tubules throughout isolation and long-term culture (Figure 4A,B). The abundance of DHPR and localization that was characteristic and unique to atrial and ventricular myocytes indicated the presences of t-tubules. Moreover, colocalization of DHPR with RYR2 immunostaining was an indicator of intact diad structures. Immunostaining for the sarcomeric protein alpha-actinin in atrial and ventricular cardiac myocytes resulted in the expected sarcomeric striation pattern. The sarcomeric striation pattern was used to assess the purity and viability of isolated cardiac myocytes in conjunction with rod-shaped morphological shape and nuclear staining with TOPRO-3 (Figure 4C,D; purple and red). As expected, ventricular cardiac myocytes were large, exhibiting an average length of ~150 mm, whereas atrial cardiac myocytes averaged ~75 mm. Furthermore, upon immunostaining analysis, atrial cardiac myocytes (but not ventricular cardiac myocytes) exhibited robust expression of atrial natriuretic peptide (ANP) in a staining pattern that was characteristic of localization to the endoplasmic reticulum and secretory granules (Figure 4C,D; green).
A characteristic unique to atrial cardiac myocytes is its classification as an endocrine cell in addition to contractile cell. While atrial myocytes secrete ANP under basal conditions, secretion increases in response to secretagogues (i.e., the alpha-adrenergic agonist, phenylephrine [PE]). Moreover, atrial cardiac myocytes secrete ANP and co-secretionally process a portion of the hormone from its precursor state (Pro-ANP, 15 kD) to the product peptide (ANP 3kD)16,17. This secretory ability can be quantified via immunoblot detection of ANP in the media of isolated atrial cardiac myocytes in response to acute PE treatment (Figure 4E). This secretory and processing ability of the atrial cardiac myocyte was found to be sensitive to culturing conditions. Thus, it is imperative that the atrial myocyte plating medium is supplemented with dexamethasone, insulin, transferrin, and selenium.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/61224/61224fig1.jpg" /> 
Figure 1: Schematic overview of retrograde heart perfusion, digestion, and cell isolation. Shown are the main steps involved in cell isolation from both atrial and ventricular chambers simultaneously from a single mouse heart. (A) A single mouse heart is rapidly cannulated via the ascending aorta and perfused in a retrograde manner. (B) The heart is separated into atrial and ventricular tissues for further digestion and physical separation. (C) Following adequate digestion, the cells are separated via gravity filtration into a total of four cellular fractions that are cultured for subsequent experimentation. <a href="https://www.jove.com/files/ftp_upload/61224/61224fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/61224/61224fig2.jpg" /> 
Figure 2: Morphological analysis of isolated atrial and ventricular cardiac myocytes and non-myocytes in culture. (A) Isolated adult mouse atrial myocytes (AMAMs), (B) adult mouse atrial non-myocytes (AMANMs), (C) adult mouse ventricular myocytes (AMVMs), or (D) adult mouse ventricular non-myocytes (AMVNMs) were plated at 5 x 105 cells/chamber on four-chamber (1.7 cm2) glass slides in respective plated media. Phase images were obtained at indicated days in culture using a 10x objective under an epifluorescence microscope. <a href="https://www.jove.com/files/ftp_upload/61224/61224fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/61224/61224fig3.jpg" /> 
Figure 3: Representative qRT-PCR analysis of isolated cell cultures. RNA was extracted from freshly isolated cardiac myocytes and non-myocytes, and mRNA levels for cell-specific gene markers were determined by qRT-PCR4. (A) Tnnt2, cardiac muscle troponin T (cardiac myocyte marker); (B) Nppa, atrial natriuretic peptide (atrial myocyte marker); (C) Myl2, myosin light chain 2 (ventricular myocyte marker); (D) Tcf21, transcription factor 21 (fibroblast marker); (E) Pdgfra, platelet-derived growth factor receptor A (fibroblast marker); (F) Cd68, cluster of differentiation 68 (monocyte-derived cell marker). Data represent mean &#177; SEM (*p &#8804; 0.05 different from all other values, as determined by ANOVA followed by Newman Keul&#8217;s post-hoc analysis). <a href="https://www.jove.com/files/ftp_upload/61224/61224fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/61224/61224fig4.jpg" /> 
Figure 4: Representative morphological and functional analysis of isolated atrial and ventricular cardiac myoyctes. (A) AMAMs or (B) AMVMs were plated at 5 x 105 cells/chamber on four-chamber (1.7 cm2) glass slides in respective plating media for 1 h to allow for adhesion. This was followed by either refeeding atrial myocyte plating media or changing to ventricular myocyte maintaining media supplemented with blebbistatin for an additional 16 h. Cultures were subsequently fixed then immunostained for RYR2 (purple), DHPR (green), and nuclear stain TOPRO-3 (red). (C) AMAMs or (D) AMVMs were isolated and plated, then immunostained for a-actinin (purple), ANP (green), and TOPRO-3 (red). Shown are two representative images for each cell type. (E) AMAMs were plated at 5 x 105 cells/well on a 12 well culture dish for 16 h in atrial myocyte plating media. AMAMs were subsequently treated for 0.5 h with vehicle or the ANP secretagogue (phenylephrine, 50 mM) before media were collected and subjected to immunoblot analysis for ANP. Prior to immunoblot analysis, media samples were centrifuged at 500 x g for 5 min to remove cellular debris and ensure that the observed ANP was the result of active secretion from AMAMs. <a href="https://www.jove.com/files/ftp_upload/61224/61224fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Simultaneous Isolation and Culture of Atrial Myocytes, Ventricular Myocytes, and Non-Myocytes from an Adult Mouse Heart at JoVE.com

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

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.

The isolation and culturing of cardiac myocytes from mice has been essential for furthering the understanding of cardiac physiology and pathophysiology. ...

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Research

JoVE Journal

Biology

7.3K Views.  San Diego State University. Een methode wordt beschreven voor de gelijktijdige isolatie van myocyten en niet-myocyten van zowel de atria als ventrikels van een enkel volwassen muizenhart. Dit protocol resulteert in consistente opbrengsten van zeer levensvatbare cardiale myocyten en niet-myocyten en beschrijft optimale celspecifieke kweekomstandigheden voor fenotyping en in vitro analyse.

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

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.

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

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+ ...

Isolation, Culture, and Functional Characterization of Adult Mouse Cardiomyoctyes

The use of primary cardiomyocytes (CMs) in culture has provided a powerful complement to murine models of heart disease in advancing our understanding of heart disease. In particular, the ability to study ion homeostasis, ion channel function, cellular excitability and excitation-contraction coupling and their alterations in diseased conditions and by disease-causing mutations have led to significant insights into cardiac diseases. Furthermore, the lack of an adequate immortalized cell line to mimic adult CMs, and the limitations of neonatal CMs (which lack many of the structural and functional biomechanics characteristic of adult CMs) in culture have hampered our understanding of the complex interplay between signaling pathways, ion channels and contractile properties in the adult heart strengthening the importance of studying adult isolated cardiomyocytes. Here, we present methods for the isolation, culture, manipulation of gene expression by adenoviral-expressed proteins, and subsequent functional analysis of cardiomyocytes from the adult mouse. The use of these techniques will help to develop mechanistic insight into signaling pathways that regulate cellular excitability, Ca2+ dynamics and contractility and provide a much more physiologically relevant characterization of cardiovascular disease.

Here we describe the isolation of adult mouse cardiomyoctyes using a Langendorff perfusion system. The resulting cells are Ca2+-tolerant, electrically quiescent and can be cultured and transfected with adeno- or lentiviruses to manipulate gene expression. Their functionality can also be analyzed using the MMSYS system and patch clamp techniques.

The use of primary cardiomyocytes (CMs) in culture has provided a powerful complement to murine models of heart disease in advancing our understanding of ...

Isolation of Atrial Myocytes from Adult Mice

The electrophysiological properties of atrial myocytes importantly affect overall cardiac function. Alterations in the underlying ionic currents responsible for the action potential can cause pro-arrhythmic substrates that underlie arrhythmias, such as atrial fibrillation, which are highly prevalent in many conditions and disease states. Isolating adult mouse atrial cardiomyocytes for use in patch-clamp experiments has greatly advanced our knowledge and understanding of the cellular electrophysiology in the healthy atrial myocardium and in the setting of atrial pathophysiology. In addition, studies using genetic mouse models have elucidated the role of a vast array of proteins in regulating atrial electrophysiology. Here we provide a detailed protocol for the isolation of cardiomyocytes from the atrial appendages of adult mice using a combination of enzymatic digestion and mechanical dissociation of these tissues. This approach consistently and reliably yields isolated atrial cardiomyocytes that can then be used to characterize cellular electrophysiology by measuring action potentials and ionic currents in patch-clamp experiments under a number of experimental conditions.

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.

The electrophysiological properties of atrial myocytes importantly affect overall cardiac function. Alterations in the underlying ionic currents ...

Medicine

Isolation and Culture of Adult Mouse Cardiomyocytes for Cell Signaling and in vitro Cardiac Hypertrophy

Technological advances have made genetically modified mice, including transgenic and gene knockout mice, an essential tool in many research fields. Adult cardiomyocytes are widely accepted as a good model for cardiac cellular physiology and pathophysiology, as well as for pharmaceutical intervention. Genetically modified mice preclude the need for complicated cardiomyocyte infection processes to generate the desired genotype, which are inefficient due to cardiomyocytes&#8217; terminal differentiation. Isolation and culture of high quantity and quality functional cardiomyocytes will dramatically benefit cardiovascular research and provide an important tool for cell signaling transduction research and drug development. Here, we describe a well-established method for isolation of adult mouse cardiomyocytes that can be implemented with little training. The mouse heart is excised and cannulated to an isolated heart system, then perfused with a calcium-free and high potassium buffer followed by type II collagenase digestion in Langendorff retrograde perfusion mode. This protocol yields a consistent result for the collection of functional adult mouse cardiomyocytes from a variety of genetically modified mice.

Isolation and Culture of Adult Mouse Cardiomyocytes for Cell Signaling and in vitro Cardiac Hypertrophy

We describe a reliable method for isolation of adult mouse cardiomyocytes. This protocol yields a consistent result for the culture of functional adult cardiomyocytes from a variety of genetically modified mice.

Technological advances have made genetically modified mice, including transgenic and gene knockout mice, an essential tool in many research fields. Adult ...

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

A single cardiomyocyte is a vital tool in the cellular and subcellular level studies of cardiac biology and diseases as a fundamental unit of contraction and electrical activity. Hence, isolating viable, high-quality cardiomyocytes from the heart is the initial and most crucial experimental step. Comparing the various protocols for isolating the cardiomyocytes of adult mice, the Langendorff retrograde perfusion is the most successful and reproducible method reported in the literature, especially for isolating ventricular myocytes. However, isolating quality atrial myocytes from the perfused heart remains challenging, and few successful isolation reports are available. Solving this complicated problem is extremely important because apart from ventricular disease, atrial disease accounts for a large part of heart diseases. Therefore, further investigations on the cellular level to reveal the mechanisms are warranted. In this paper, a protocol based on the Langendorff retrograde perfusion method is introduced and some modifications in the depth of aorta cannulation and the steps that may affect the digestion process to isolate atrial and ventricular myocytes were simultaneously made. Moreover, the isolated cardiomyocytes are confirmed to be amenable to patch clamp investigation.

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.

A single cardiomyocyte is a vital tool in the cellular and subcellular level studies of cardiac biology and diseases as a fundamental unit of contraction ...

Isolation, Culture and Transduction of Adult Mouse Cardiomyocytes

Cultured cardiomyocytes can be used to study cardiomyocyte biology using techniques that are complementary to in vivo systems. For example, the purity and accessibility of in vitro culture enables fine control over biochemical analyses, live imaging, and electrophysiology. Long-term culture of cardiomyocytes offers access to additional experimental approaches that cannot be completed in short term cultures. For example, the in vitro investigation of dedifferentiation, cell cycle re-entry, and cell division has thus far largely been restricted to rat cardiomyocytes, which appear to be more robust in long-term culture. However, the availability of a rich toolset of transgenic mouse lines and well-developed disease models make mouse systems attractive for cardiac research. Although several reports exist of adult mouse cardiomyocyte isolation, few studies demonstrate their long-term culture. Presented here, is a step-by-step method for the isolation and long-term culture of adult mouse cardiomyocytes. First, retrograde Langendorff perfusion is used to efficiently digest the heart with proteases, followed by gravity sedimentation purification. After a period of dedifferentiation following isolation, the cells gradually attach to the culture and can be cultured for weeks. Adenovirus cell lysate is used to efficiently transduce the isolated cardiomyocytes. These methods provide a simple, yet powerful model system to study cardiac biology.

This protocol describes a step-by-step method for the reproducible isolation and long-term culture of adult mouse cardiomyocytes with high yield, purity, and viability.

Cultured cardiomyocytes can be used to study cardiomyocyte biology using techniques that are complementary to in vivo systems. For example, the purity and ...

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.

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

A Simple and Effective Method to Consistently Isolate Mouse Cardiomyocytes

The need for reproducible yet technically simple methods yielding high-quality cardiomyocytes is essential for research in cardiac biology. Cellular and molecular functional experiments (e.g., contraction, electrophysiology, calcium cycling, etc.) on cardiomyocytes are the gold standard for establishing mechanism(s) of disease. The mouse is the species of choice for functional experiments and the described technique is specifically for the isolation of mouse cardiomyocytes. Previous methods requiring a Langendorff apparatus require high levels of training and precision for aortic cannulation, often resulting in ischemia. The field is shifting toward Langendorff-free isolation methods that are simple, are reproducible, and yield viable myocytes for physiological data acquisition and culture. These methods greatly diminish ischemia time compared to aortic cannulation and result in reliably obtained cardiomyocytes. Our adaptation to the Langendorff-free method includes an initial perfusion with ice-cold clearing solution, use of a stabilizing platform that ensures a steady needle during perfusion, and additional digestion steps to ensure reliably obtained cardiomyocytes for use in functional measurements and culture. This method is simple and quick to perform and requires little technical skill.

The gold standard in cardiology for cellular and molecular functional experiments are cardiomyocytes. This article describes adaptations to the non-Langendorff technique to isolate mouse cardiomyocytes.

The need for reproducible yet technically simple methods yielding high-quality cardiomyocytes is essential for research in cardiac biology. Cellular and ...

Simultaneous Isolation of High Quality Cardiomyocytes, Endothelial Cells, and Fibroblasts from an Adult Rat Heart

The rat is an important animal model used in cardiovascular research, and rat cardiac cells are used routinely for in vitro analysis of the molecular mechanisms of cardiovascular disease progression such as cardiac hypertrophy, fibrosis, and atherosclerosis. Although several attempts with variable success have been made to develop immortalized cell lines from the cardiovascular system to understand these cellular mechanisms, primary cells offer a more natural and close to in vivo environment for such studies. Therefore, different laboratories working on a particular cell type have developed protocols to isolate individual types of rat cardiac cells of interest. A protocol that allows the isolation of more than one cell type, however, is missing. Here an optimized protocol is described that allows the isolation of high-quality major cardiac cell types (cardiomyocytes, endothelial cells, and fibroblasts) from a single preparation and enables their use for cellular analyses. This permits the most efficient use of available resources, which may save time and reduce research costs.

Several protocols have been developed and described for the isolation of different cardiac cell types from a rat heart. Here, an optimized protocol is described that allows the isolation of high-quality major cardiac cell types (cardiomyocytes, endothelial cells, and fibroblasts) from a single preparation, reducing the experimental costs.

The rat is an important animal model used in cardiovascular research, and rat cardiac cells are used routinely for in vitro analysis of the molecular ...

An Antegrade Perfusion Method for Cardiomyocyte Isolation from Mice

In basic research using mouse heart, isolating viable individual cardiomyocytes is a crucial technical step to overcome. Traditionally, isolating cardiomyocytes from rabbits, guinea pigs or rats has been performed via retrograde perfusion of the heart with enzymes using a Langendorff apparatus. However, a high degree of skill is required when this method is used with a small mouse heart. An antegrade perfusion method that does not use a Langendorff apparatus was recently reported for the isolation of mouse cardiomyocytes. We herein report a complete protocol for the improved antegrade perfusion of the excised heart to isolate individual heart cells from adult mice (8 - 108 weeks old). Antegrade perfusion is performed by injecting perfusate near the apex of the left ventricle of the excised heart, the aorta of which was clamped, using an infusion pump. All procedures are carried out on a pre-warmed heater mat under a microscope, which allows for the injection and perfusion processes to be monitored. The results suggest that ventricular and atrial myocytes, and fibroblasts can be well isolated from a single adult mouse simultaneously.

We developed a simple method for isolating high quality individual mouse heart cells by the antegrade perfusion technique. This method is Langendorff-free and useful for isolating ventricular and atrial myocytes or interstitial cells, such as cardiac fibroblasts or progenitors.

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

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