The authors gratefully acknowledge Ms. Cynthia DeKay for the preparation of the figures.

All mouse experiments were performed in accordance with US Animal Welfare Act and were approved by the Institutional Animal Care and Use Committee at the University of Minnesota.
1. Method for Mouse Heart Isolation
<ol>
	<li>Euthanize a neonatal mouse by decapitation with a single use blade.</li>
	<li>Swab the thorax with 70% ethanol.</li>
	<li>Dissect the skin from the chest by cutting it away from the chest wall with standard scissors while pulling the skin laterally with a pair of #5 forceps.</li>
	<li>Perforate the abdomen just inferior to the sternum with the scissors by cutting through the abdominal wall. Grasping the xiphoid process with #5 forceps, retract the sternum rostrally from the body while cutting though the ribs on either side of the chest with the scissors. The rib cage is reflected superiorly with the forceps to reveal the heart.</li>
	<li>Bluntly dissect the two main lobes of the thymus by pulling laterally with #5 forceps, exposing the arch of the aorta, as well as the caval and pulmonary veins.</li>
	<li>Transect the major arteries from the aortic arch, and the aorta itself, with the 10 cm spring scissors. Retain the aorta between the base of the heart and the brachiocephalic artery. Grasp the ends of the severed vessels with the #5 forceps to reflect the heart forward, separating it from the trachea and esophagus.</li>
	<li>Transect the pulmonary vasculature and other major veins, by cutting between the lungs and the heart on both sides of the heart with the 10 cm spring scissors. The veins remain open to provide drainage.</li>
	<li>Remove the heart from the mediastinum with the #5 forceps, grasping the severed ends of the major vessels. Place the heart in a 60 mm culture dish containing sterile phosphate buffered saline (PBS) for catheterization.</li>
</ol>
2. Method for Decellularization by Langendorff Perfusion
<ol>
	<li>Prepare the catheter assembly in advance. Draw a 4 cm section of PE 50 tubing in a small alcohol flame to create a smaller, thinner catheter. Trim the ends with a blade to meet the dimensions (Approx. 300 &#181;m outside diameter O.D. with a flange of approx. 500 &#181;m O.D.) shown in Figure 1. This will provide two symmetrical catheters from each side of the pull.</li>
	<li>Point the cut end of the tubing into the flame briefly, to melt a flange onto the opening at the thin end.</li>
	<li>Fill the 12 ml syringe with PBS and assemble the catheter by placing a 3-way stopcock on the syringe. Add a 22 G x 1 needle to the stopcock and drive the needle through the septum. Slide the drawn PE tubing catheter onto the needle (Fig. 1).</li>
	<li>Irrigate the assembled parts with PBS, assuring that all air bubbles have been removed.</li>
	<li>Insert the catheter, prepared as outlined above, into the aorta of the isolated heart, not extending past the aortic valve and ligate with one tie of 7-0 suture. Rest the flange of the catheter proximally against the tie, making a tight seal and preventing the heart from coming off the catheter.</li>
	<li>Observe the catheterization under magnification, while gently perfusing the heart using the syringe containing PBS. Ensure that there are no leaks in the system and the tissue homogeneously blanches as latent blood is removed.</li>
	<li>Place the septum into the neck of the inlet adaptor and seal it by folding the sides over the glass.</li>
	<li>Attach the reservoir filled with 60 ml of 1% sodium dodecyl sulfate (SDS) in distilled water (dH2O) via a line of sufficient length to produce a column that generates 20 mm Hg pressure as shown in Fig. 1. Calculate the pressure from the liquid column height based on the relationship of 1 mm Hg is equal to 1.3595 cm H2O. 
	Caution: SDS is a highly flocculent powder with irritant properties. Contact should be avoided. Handle the powder using appropriate protective clothing.</li>
	<li>Perfuse the heart with 1% SDS for 14 hr. The heart will be translucent in appearance with no observable remaining tissue.</li>
	<li>Flush the system up to the stopcock of the remaining SDS solution and replace it with 10 ml dH2O. Perfuse the heart with 10 ml 1% Triton X-100 (diluted in distilled water), followed by 10 ml dH2O, followed by 60 ml PBS containing 1x penicillin streptomycin (Pen-Strep).</li>
	<li>Store the heart in PBS with 1x Pen-Strep at 4 &#176;C. If the intended post decellularization application requires perfusion then the catheter in the aorta should be maintained, otherwise cut the suture tie and remove the catheter.</li>
</ol>
3. DNA Determination
<ol>
	<li>Prepare a digest of the decellularized ECM or control heart using 200 &#956;g/ml proteinase K in 50 mM KCl, 2.5 mM MgCl2, 0.45% Tween 20 in 10 mM Tris (pH 8.3).</li>
	<li>Incubate the tissue at 55 &#176;C with agitation until the tissue is dissolved, typically 4-5 hr.</li>
	<li>Quantitate the DNA content of the homogenate with a DNA binding assay4,11.</li>
</ol>
4. Fixation and Sectioning of Tissue
<ol>
	<li>Fix decellularized, recellularized or control P3 hearts in 4% paraformaldehyde in PBS for 30 min at room temperature.</li>
	<li>Wash the tissue in PBS 3x.</li>
	<li>Place the tissue in a solution of 7.5% sucrose in 0.1 M phosphate buffer at 4 &#176;C until it sinks.</li>
	<li>Change the solution to 15% sucrose in 0.1 M phosphate buffer at 4 &#176;C, again, until it sinks.</li>
	<li>Warm the tissue to 37 &#176;C, replace half of the volume with gelatin solution in 15% sucrose &#38; 0.1 M phosphate buffer and equilibrate overnight. Concentrations of gelatin are increased stepwise through 1%, 2.5%, 5% and finally 7.5% twice.</li>
	<li>Place the samples in cryomolds using fresh 7.5% gelatin. To restore the shape of the decellularized samples, liquid gelatin can be perfused into the chambers as the hearts are molded. Freeze by floating the cryomolds on liquid nitrogen. Store at -80 &#176;C.</li>
	<li>Cut (10 &#181;m thick) sections with a cryostat. Bring the slide close to the section surface and observe the section move off from the knife onto the surface due to the charge on the electrostatically treated slides. Dry the slides overnight and store at -80 &#176;C for future analysis.</li>
	<li>Remove the slides from the freezer, equilibrate to room temperature and then place in a Coplin jar containing PBS for 20 min at 37 &#176;C to dissolve the gelatin.</li>
	<li>Stain the cut sections from Step 4.7 with Hematoxylin and Eosin. Place slides in a Coplin jar. Expose the slides hydrated in Step 4.8 to Hematoxylin for 45 sec, tap water for 1.5 min, buffer for 3 min, tap water for 1 min, bluing agent for 1.5 min, 80% ethanol for 1 min, Alcoholic Eosin Y for 8 sec, 80% ethanol for 1 min, 100% ethanol for 1 min 2x, clearing agent (xylene substitute) for 1 min 3x, coverslip with resin based mounting medium. Examine the slides microscopically.</li>
	<li>To confirm the retention of ECM protein reactivity of the heart ECM, stain for ECM structural proteins such as collagen IV by placing the hydrated slides in a humidified chamber and treat with 10% normal donkey serum (NDS) in phosphate buffered saline with 0.1% Triton-X100 (PBST) for 1 hr at room temperature (RT). Use a sufficient volume to cover the tissue sections.</li>
	<li>Replace the solution with the primary antibody of choice at an empirically determined dilution in 5% NDS / PBST. For example, the Collagen IV antibody was diluted at 1:150. Incubate overnight at 4 &#176;C.</li>
	<li>Wash the slides with PBST 3x and apply a secondary antibody of choice conjugated with a fluorescent dye. Dilute the antibody by an empirically determined amount. Incubate for 1 hr at RT. Wash with PBS 3x.</li>
	<li>Stain the slides with a DNA binding dye such as DAPI to verify absence of cell nuclei by using a DAPI containing mounting medium when cover slipping the slides.</li>
	<li>Examine the slides with a fluorescent microscope at 50 to 400X.</li>
</ol>
5. P1 Neonatal Murine Ventricular Cardiomyocytes for Recellularization
<ol>
	<li>Spray each pup with 70% ethanol and decapitate with a single use blade.</li>
	<li>Hold each pup between the thumb and forefinger while the thorax is split at the midline with small sterile scissors to expose the thoracic cavity. Apply pressure to allow the heart to protrude freely from the chest while it is cut free of the major vessels and the atria leaving only the ventricular tissue.</li>
	<li>Place each heart directly into a 50 ml tube containing 20 ml ice-cold Calcium, Bicarbonate free Hank&#39;s buffered saline solution with 20 mM 4-(2-hydroxyethyl)-1-piperazineethanesulfonic acid (CBFHH) until all the hearts are collected.</li>
	<li>Aspirate the CBFHH and add 10-15 ml of fresh CBFHH (ice-cold) to the tube. Wash the tissue by swirling the tissue in the tube several times.</li>
	<li>Decant the solution containing the hearts into a 60 mm plastic Petri dish.</li>
	<li>Dissect any latent atrial tissue from the hearts under magnification on ice by trimming it away from the hearts with the spring scissors. Mince up the ventricles into homogenously sized small pieces. Remove any separated non-ventricular tissue from the dish with #5 forceps.</li>
	<li>Pipet as much of the CBFHH solution as is needed to transfer the tissue fragments into a small sterile vial that contains a sterile micro stir bar.</li>
	<li>Allow the tissue to sediment to the bottom of the vial and remove the CBFHH solution.</li>
	<li>Make up 50 ml of an enzyme solution 1.75 mg/ml trypsin, 20 &#181;g/ml DNase II in CBFHH. Pipet 5 ml of this enzyme solution and add it to a tube containing minced ventricular tissue and place on a magnetic stirrer. Stir at a constant rate (340 rpm) at room temperature for 8 min. 
	NOTE: The stirring action should be gentle and yet allow for the suspension of the slurry.</li>
	<li>Remove the vial from the stir plate and allow the slurry to sediment for 3 min. Pipet and discard the initial digest supernatant, as it primarily contains blood cells and tissue debris.</li>
	<li>Pipet a second 5 ml aliquot of the enzyme solution and add it to the digesting ventricle. Stir for 8 min and allow it to sediment for another 3 min. Prior to beginning the digests, prepare two 50 ml tubes (labeled 1 and 2) each containing 12 ml ice-cold fetal bovine serum (FBS). Place a 40 &#181;m cell strainer atop each tube. Pipet this supernatant through the filter on tube 1.</li>
	<li>Repeat the digestion process an additional 8 times, alternating the placement of the digest supernatant between the two tubes containing FBS. Split the last supernatant equally between tubes 1 and 2 to ensure equal volumes in each tube. 
	NOTE: Each collection tube will now contain 32.5 ml total volume of cell suspension.</li>
	<li>Centrifuge the tubes containing the supernatant 150 x g for 6 min at 4 &#176;C.</li>
	<li>While collecting the digestion aliquots, prepare five 100 mm tissue culture plates with 6 ml of media (Dulbecco&#39;s Modified Eagle&#39;s Media (DMEM) with 10% FBS, 1x Pen-Strep, 1x L-glutamine) per plate. Incubate these aliquots at 37 &#176;C, 5% CO2 for 30 min to equilibrate the media.</li>
	<li>Aspirate the CBFHH enzyme mixture and resuspend the cells into the 30 ml of culture media prepared above, combining the cells from both collection tubes.</li>
	<li>Return 6 ml of cell suspension to each of the 100 mm plates and incubate for 45 min at 37 &#176;C.</li>
	<li>At the end of the incubation, transfer the non-adherent cells to 5 new dishes and re-incubate for 45 min (the fibroblast fraction will have begun to adhere to the dishes and can be grown out separately if desired).</li>
	<li>At the end of the second round of pre-plating, collect the media and non-adherent cells from the dishes and spin the media at 150 x g for 6 min.</li>
	<li>Draw off excess media to bring the cells to the approximate desired concentration, (4.0 x 105 cells per construct in 100 &#181;l of perfusate). Remove an aliquot for counting and or viability testing14.</li>
</ol>
6. Bioreactor Recellularization of P3 Heart Matrix
<ol>
	<li>Pretreat the isolated heart matrix with culture media (see Step 5.15) overnight before adding the cells.</li>
	<li>Assemble the elements of a Langendorff system as shown in Fig. 2. Autoclave the glass parts and ethylene oxide sterilize the plastic parts to assure sterility. Various sub units of the system can be assembled in a laminar flow hood before being mounted on the support stand. Circulating water bath and heated water flow path has been omitted for clarity.</li>
	<li>Fill the assembled system with 120 ml of tissue culture media (see Step 5.15).</li>
	<li>Place the catheterized heart matrix from Step 2.14 in a 60 mm culture dish under magnification and connect a 1 ml syringe with 22 G x 1 needle loaded with cell suspension from Step 5.20 to the catheter. Ensure that this assembly is free of air bubbles to avoid embolizing the heart.</li>
	<li>Gently perfuse the 100 &#181;l of cell suspension into the heart matrix via the coronary arteries. Once complete, detach the syringe/needle combination. 
	NOTE: A slow perfusion of approx. 20 &#181;l per min is required to prevent the cells from flowing out of the veins, transiting the heart.</li>
	<li>With a 22g blunt stub secured to the Luer fitting on the underside of the bioreactor heart jar lid, push the catheter onto the stub.</li>
	<li>Start the peristaltic pump and observe that the flow proceeds as outlined in Figure 2. Flow proceeds from the reservoir via the pump through the bubble trap to the catheter placed in the aorta in Step 2.5 (red path in Fig. 2). Observe the flow of the cardiac circulation out of the veins and drip from the apex, recirculating to the media reservoir. 
	NOTE: The perfusion flow rate is dependent on individual factors such as the vascular resistance of the construct, and the size of the heart, but a rate of 50 to 100 &#181;l/min is a good starting point. At intermediate time points, functional assessments can be executed. The size scale of the neonatal recellularized heart limits the assessments, that can be performed but we have determined that optically based systems can be used to quantify beating behavior just as they have been used in adult rat hearts.4 The construct can be perfused for extended periods of time (up to 23 hr).</li>
</ol>

<ol>
	<li>Yusen, R. D., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Registry+of+the+International+Society+for+Heart+and+Lung+Transplantation:+Thirty-second+official+adult+lung+and+heart-lung+transplantation+report--2015.">Registry of the International Society for Heart and Lung Transplantation: Thirty-second official adult lung and heart-lung transplantation report--2015.</a> J Heart Lung Transplant. 34 (10), 1264-1277 (2015).</li><li>Go, A. S., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Heart+disease+and+stroke+statistics--2014+update:+A+report+from+the+american+heart+association.">Heart disease and stroke statistics--2014 update: A report from the american heart association.</a> Circulation. 129 (3), e28-e292 (2014).</li><li>Kapelios, C. J., Nanas, J. N., Malliaras, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Allogeneic+cardiosphere-derived+cells+for+myocardial+regeneration:+current+progress+and+recent+results.">Allogeneic cardiosphere-derived cells for myocardial regeneration: current progress and recent results.</a> Future Cardiol. 12 (1), 87-100 (2016).</li><li>Ott, H. C., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Perfusion+decellularized+matrix:+Using+nature's+platform+to+engineer+a+bioartificial+heart.">Perfusion decellularized matrix: Using nature's platform to engineer a bioartificial heart.</a> Nat Med. 14 (2), 213-221 (2008).</li><li>Porrello, E. R., Olson, E. O. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+neonatal+blueprint+for+cardiac+regeneration.">A neonatal blueprint for cardiac regeneration.</a> Stem Cell Research. 13 (3 Pt B), 556-570 (2014).</li><li>Porrello, E. R., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Transient+regenerative+potential+of+the+neonatal+mouse+heart.">Transient regenerative potential of the neonatal mouse heart.</a> Science. 331 (6020), 1078-1080 (2011).</li><li>Polizzotti, B. D., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Neuregulin+stimulation+of+cardiomyocyte+regeneration+in+mice+and+human+myocardium+reveals+a+therapeutic+window.">Neuregulin stimulation of cardiomyocyte regeneration in mice and human myocardium reveals a therapeutic window.</a> Sci Transl Med. 7 (281), 281ra45 (2015).</li><li>Jesty, S. A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=c-kit++precursors+support+postinfarction+myogenesis+in+the+neonatal,+but+not+adult,+heart.">c-kit+ precursors support postinfarction myogenesis in the neonatal, but not adult, heart.</a> Proc Natl Acad Sci U S A. 109 (33), 13380-13385 (2012).</li><li>Ambrosy, A. P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+Global+Health+and+Economic+Burden+of+Hospitalizations+for+Heart+Failure:+Lessons+Learned+From+Hospitalized+Heart+Failure+Registries.">The Global Health and Economic Burden of Hospitalizations for Heart Failure: Lessons Learned From Hospitalized Heart Failure Registries.</a> J Am Coll Cardiol. 63 (12), 1123-1133 (2014).</li><li>Roger, V. L., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Executive+Summary:+Heart+Disease+and+Stroke+Statistics-2012+Update+A+Report+From+the+American+Heart+Association.">Executive Summary: Heart Disease and Stroke Statistics-2012 Update A Report From the American Heart Association.</a> Circulation. 125 (22), 188-197 (2012).</li><li>Kennedy-Lydon, T., Rosenthal, N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Cardiac+regeneration:+epicardial+mediated+repair.">Cardiac regeneration: epicardial mediated repair.</a> Proc R Soc B. 282 (1821), 2147-2172 (2015).</li><li>Williams, C., Sullivan, K., Black, L. D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Partially+Digested+Adult+Cardiac+Extracellular+Matrix+Promotes+Cardiomyocyte+Proliferation+In+Vitro.">Partially Digested Adult Cardiac Extracellular Matrix Promotes Cardiomyocyte Proliferation In Vitro.</a> Adv Healthcare Mat. 4 (10), 1545-1554 (2015).</li><li>Borg, T. K., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Recognition+of+extracellular+matrix+components+by+neonatal+and+adult+cardiac+myocytes.">Recognition of extracellular matrix components by neonatal and adult cardiac myocytes.</a> Dev Biol. 104 (1), 86-96 (1984).</li><li>Strober, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Trypan+blue+exclusion+test+of+cell+viability.">Trypan blue exclusion test of cell viability.</a> Curr Protoc Immnol. 111, A3-B1-3 (2015).</li><li>Gilbert, T. W., Freund, J. M., Badylak, S. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Quantification+of+DNA+in+biologic+scaffold+materials.">Quantification of DNA in biologic scaffold materials.</a> J Surg Res. 152 (1), 135-139 (2009).</li><li>Akhyari, P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+quest+for+an+optimized+protocol+for+whole-heart+decellularization:+a+comparison+of+three+popular+and+a+novel+decellularization+technique+and+their+diverse+effects+on+crucial+extracellular+matrix+qualities.">The quest for an optimized protocol for whole-heart decellularization: a comparison of three popular and a novel decellularization technique and their diverse effects on crucial extracellular matrix qualities.</a> Tissue Eng Part C Methods. 17 (9), 915-926 (2011).</li><li>Lu, T. Y., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Repopulation+of+decellularized+mouse+heart+with+human+induced+pluripotent+stem+cell-derived+cardiovascular+progenitor+cells.">Repopulation of decellularized mouse heart with human induced pluripotent stem cell-derived cardiovascular progenitor cells.</a> Nat Commun. 4 (2307), 1-11 (2013).</li></ol>

The authors have nothing to disclose.

The dependence of this technique on repeated perfusions of the heart makes the avoidance of an embolism a critical component of a successful outcome. From the initial catheterization of the heart in Steps 2.2-2.6, to the changes of solution between Steps 2.8-2.14, there are manipulations that can allow introduction of air bubbles which compromise the flow of perfusate into the myocardium. Due to the diminutive size of the neonatal heart, even minute bubbles in the vasculature can cause a technical infarct, thus rendering...

Heart failure is common and deadly. It is a progressive disease that results in decreased contractility of the heart, which impairs blood flow to organs and leaves the metabolic demands of the body unmet. It is estimated that 5.7 million Americans have heart failure and it is the primary cause of hospitalization in the United States9. The collective cost of treating patients in heart failure in the United States exceeds $300 billion dollars per year 9-10. The only definitive therapy for end stage heart failure is orthotopic heart transplantation. Each year, it is estimated that more than 100,000 donor hearts are needed for cardiac transplantation procedures in the United States1-2. Due to the limited numbers of donors, only approximately 2,400 transplants are performed each year in the U.S.2. Clearly, this organ shortage needs to be addressed as other strategies are required to produce additional organs for transplantation and, ideally, these organs would be autologous so as to avoid the complications associated with rejection and lifetime immunosuppression.
Mammalian adult cardiomyocytes demonstrate a limited regenerative capacity upon injury but recent evidence suggests that mammalian neonatal hearts maintain a remarkable regenerative capacity following injury5-8. Specifically, following partial surgical resection, a regenerative window has been discovered between birth and postnatal day 7. This regenerative period is characterized by a lack of fibrotic scar, formation of neovascularization, release of angiogenic factors from the epicardium, and cardiomyocyte proliferation 5-8,11. This regenerative window of time provides the potential for using the neonatal heart as a novel source of material for the development of a bioartificial heart.
The extracellular matrix is known to provide important cues to promote cardiomyocyte proliferation and growth. Distinct differences in the availability of molecules in the neonatal and adult matrices12 and their ability to promote regeneration have been explored13. Decellularized adult matrices have been used in several studies to provide an ECM scaffold for cellular repopulation and the generation of a bioartificial heart. While these studies, and new discoveries in stem cell technologies, are advancing rapidly, several hurdles have yet to be met. For example, limitations in preserving native structure of the matrix, cellular integration into the matrix wall, and ability to support proliferation and growth all limit the success of this approach. While superior regenerative attributes have been ascribed to the neonatal heart, the practical aspects of using such a tissue have limited its exploration.
Based on the demonstrated regenerative capacity of the neonatal heart, we have developed novel matrices by developing a technique of decellularization for the P3 mouse heart. The P3 heart was chosen for these studies as it is within the window of cardiac regeneration as previously determined6 but the heart is large enough to harvest, decellularize and recellularize. The goal of this study is to demonstrate the feasibility of creating a matrix from a neonatal mouse heart. Our studies provide evidence for the feasibility of decellularizing a minute, neonatal heart while maintaining the structural and proteinaceous integrity of the ECM. We also demonstrate the ability to recellularize this cardiac ECM with mCherry expressing cardiomyocytes and we have examined these cardiomyocytes for expression of various cardiac markers following recellularization. This technology will allow for the testing of the superiority of a neonatal matrix for the development of a bioartificial heart.

<table><tbody><tr><td colspan="4">&lt;strong&gt;1. Materials for mouse heart isolation&lt;/strong&gt;</td></tr><tr><td>P1 mouse pups (as shown; B6;D2-Tg(Myh6*-mCherry)2Mik/J)</td><td>Jackson Laboratories</td><td>21577</td><td>or equivalent</td></tr><tr><td>60 mm Culture dish</td><td>BD Falcon</td><td>353004</td><td>or equivalent</td></tr><tr><td>Phosphate buffered saline pH 7.4 (sterile)</td><td>Hyclone</td><td>SH30256.01</td><td>or equivalent</td></tr><tr><td>Single Use Blade</td><td>Stanley</td><td>28-510</td><td>or equivalent</td></tr><tr><td>Standard Scissors</td><td>Moria Bonn (Fine Science Tools)</td><td>14381-43</td><td>or equivalent</td></tr><tr><td>Spring Scissors 10 cm</td><td>Fine Science Tools</td><td>15024-10</td><td>or equivalent</td></tr><tr><td>Vannas Spring Scissors - 3 mm Cutting Edge</td><td>Fine Science Tools</td><td>15000-00</td><td>or equivalent</td></tr><tr><td>#5 Forceps</td><td>Dumnot (Fine Science Tools)</td><td>11295-00</td><td>or equivalent</td></tr><tr><td colspan="4">&lt;strong&gt;2. Materials for decellularization&lt;/strong&gt;</td></tr><tr><td>Inlet adaptor</td><td>Chemglass</td><td>CG-1013</td><td>autoclavable</td></tr><tr><td>Septum</td><td>Chemglass</td><td>CG-3022-99</td><td>autoclavable</td></tr><tr><td>1/8 in. ID x 3/8 OD C-Flex tubing</td><td>Cole-Parmer</td><td>EW-06422-10</td><td>autoclavable</td></tr><tr><td>Male luer to 1/8&quot; hose barb adaptor</td><td>McMaster-Carr</td><td>51525K33</td><td>autoclavable</td></tr><tr><td>Female luer to 1/8&quot; hose barb adaptor</td><td>McMaster-Carr</td><td>51525K26</td><td>autoclavable</td></tr><tr><td>Prolene 7-0 surgical suture&amp;nbsp;</td><td>Ethicon</td><td>8648G</td><td>or equivalent</td></tr><tr><td>Ring stand</td><td>Fisher Scientific</td><td>S47807</td><td>or equivalent</td></tr><tr><td>Clamp</td><td>Fisher Scientific</td><td>05-769-6Q</td><td>or equivalent</td></tr><tr><td>Clamp regular holder</td><td>Fisher Scientific</td><td>05-754Q</td><td>or equivalent</td></tr><tr><td>60 cc syringe barrel&amp;nbsp;</td><td>Coviden</td><td>1186000777T</td><td>or equivalent</td></tr><tr><td>Beaker</td><td>Kimble</td><td>14000250</td><td>or equivalent</td></tr><tr><td>22 G x 1 Syringe Needle</td><td>BD</td><td>305155</td><td>or equivalent</td></tr><tr><td>12 cc syringe</td><td>Coviden</td><td>8881512878</td><td>or equivalent</td></tr><tr><td>3-way stop cock</td><td>Smith Medical</td><td>MX5311L</td><td>or equivalent</td></tr><tr><td>PE50 tubing</td><td>BD Clay Adams Intramedic</td><td>427411</td><td>Must be formable by heat. Polyethylene recommended.</td></tr><tr><td>1% SDS</td><td>Invitrogen</td><td>15525-017</td><td>Ultrapure grade recommended. Make up fresh solution and filter sterilize before use.</td></tr><tr><td>1% Triton X-100&amp;nbsp;</td><td>Sigma-Aldrich</td><td>T8787</td><td>Make up fresh solution from a 10% stock and filter sterilize before use.&amp;nbsp;</td></tr><tr><td>Sterile dH&lt;sub&gt;2&lt;/sub&gt;O</td><td>Hyclone</td><td>SH30538.02</td><td>Or MilliQ system purified water.</td></tr><tr><td>1x Pen/Strep</td><td>Corning CellGro</td><td>30-001-Cl</td><td>or equivalent&lt;br /&gt;&amp;nbsp;</td></tr><tr><td colspan="4">&lt;strong&gt;3. Materials for DNA quantitation&lt;/strong&gt;</td></tr><tr><td>Proteinase K</td><td>Fisher</td><td>BP1700</td><td>&gt;30 U/mg activity</td></tr><tr><td>KCl</td><td>Sigma-Aldrich</td><td>P9333</td><td>or equivalent</td></tr><tr><td>MgCl&lt;sub&gt;2&lt;/sub&gt;&amp;#183;6H&lt;sub&gt;2&lt;/sub&gt;O</td><td>Mallinckrodt</td><td>5958-04</td><td>or equivalent</td></tr><tr><td>Tween 20&amp;nbsp;</td><td>Sigma-Aldrich</td><td>P1379</td><td>or equivalent</td></tr><tr><td>Tris base/hydrochloride</td><td>Sigma-Aldrich</td><td>T1503/T5941</td><td>or equivalent</td></tr><tr><td>Pico-Green dsDNA assay kit</td><td>Life Technologies&amp;nbsp;</td><td>P7589</td><td>requires fluorimeter to read</td></tr><tr><td colspan="4">&lt;strong&gt;4. Method for fixation and sectioning of tissue&lt;/strong&gt;</td></tr><tr><td>Paraformaldehyde</td><td>Sigma-Aldrich</td><td>P6148</td><td>or equivalent</td></tr><tr><td>Gelatin Type A from porcine skin</td><td>Sigma-Aldrich</td><td>G2500</td><td>must be 300 bloom or greater</td></tr><tr><td colspan="4">&lt;strong&gt;5. Method for tissue histology&lt;/strong&gt;</td></tr><tr><td>Cryomolds 10 x 10 x 5 mm</td><td>Tissue-Tek</td><td>4565</td><td>or equivalent</td></tr><tr><td>Cryostat</td><td>Hacker/Bright</td><td>Model OTF</td><td>or equivalent</td></tr><tr><td>Microscope Slides&amp;nbsp; 25 x 75 x 1 mm</td><td>Fisher Scientific</td><td>12-550-19</td><td>or equivalent</td></tr><tr><td>Hematoxylin 560&amp;nbsp;</td><td>Surgipath/Leica Selectech&amp;nbsp;</td><td>3801570</td><td>or equivalent</td></tr><tr><td>Ethanol</td><td>Decon Laboratories</td><td>2701</td><td>or equivalent</td></tr><tr><td>Define</td><td>Surgipath/Leica Selectech&amp;nbsp;</td><td>3803590</td><td>or equivalent</td></tr><tr><td>Blue buffer&amp;nbsp;</td><td>Surgipath/Leica Selectech&amp;nbsp;</td><td>3802915</td><td>or equivalent</td></tr><tr><td>Alcoholic Eosin Y 515&amp;nbsp;</td><td>Surgipath/Leica Selectech&amp;nbsp;</td><td>3801615</td><td>or equivalent</td></tr><tr><td>Formula 83 Xylene substitute&amp;nbsp;</td><td>CBG Biotech&amp;nbsp;</td><td>CH0104B</td><td>or equivalent</td></tr><tr><td>Permount Mounting Medium&amp;nbsp;</td><td>Fisher Chemical&amp;nbsp;</td><td>SP15-500</td><td>or equivalent</td></tr><tr><td>Collagen IV Antibody</td><td>Rockland</td><td>600-401-106.1</td><td>or equivalent</td></tr><tr><td>&amp;alpha;-Actinin Antibody</td><td>Abcam</td><td>AB9465</td><td>or equivalent</td></tr><tr><td>mCherry Antibody</td><td>Abcam</td><td>AB205402</td><td>or equivalent</td></tr><tr><td>NKX2.5 Antibody</td><td>Santa Cruz Biotechnology</td><td>SC-8697</td><td>or equivalent</td></tr><tr><td>Donkey anti-mouse AF488 Antibody</td><td>Life Technology</td><td>A21202</td><td>or equivalent</td></tr><tr><td>Donkey anti-chicken AF594 Antibody</td><td>Jackson Immunoresearch</td><td>703-585-155&amp;nbsp;</td><td>or equivalent</td></tr><tr><td>Donkey anti-goat CY5 Antibody</td><td>Jackson Immunoresearch&amp;nbsp;</td><td>705-175-147</td><td>or equivalent</td></tr><tr><td>Fab Fragment Goat Anti-Rabbit IgG (H+L) AF594</td><td>Jackson Immunoresearch</td><td>111-587-003</td><td>or equivalent</td></tr><tr><td>Prolong Gold Antifade Mountant with DAPI</td><td>ThermoFisher</td><td>P36930</td><td>or equivalent</td></tr><tr><td colspan="4">&lt;strong&gt;6. Isolation of neonatal ventricular cardiomyocytes using pre-plating&lt;/strong&gt;</td></tr><tr><td>HBSS (Ca, Mg Free)</td><td>Hyclone</td><td>SH30031.02</td><td>or equivalent</td></tr><tr><td>HEPES (1 M)</td><td>Corning CellGro</td><td>25-060-Cl</td><td>or equivalent</td></tr><tr><td>Cell Strainer</td><td>BD Falcon</td><td>352340</td><td>or equivalent</td></tr><tr><td>50 ml tube</td><td>BD Falcon</td><td>352070</td><td>or equivalent</td></tr><tr><td>Primeria 100 mm plates</td><td>Corning</td><td>353803</td><td>Primeria surface enhances fibroblast attachment promoting a higher myocyte purity</td></tr><tr><td>Trypsin</td><td>Difco</td><td>215240</td><td>or equivalent</td></tr><tr><td>DNase II</td><td>Sigma-Aldrich</td><td>D8764</td><td>or equivalent</td></tr><tr><td>DMEM (Delbecco&#039;s Minimal Essential Media)</td><td>Hyclone</td><td>SH30022.01</td><td>or equivalent</td></tr><tr><td>Vitamin B12&amp;nbsp;</td><td>Sigma-Aldrich</td><td>V6629</td><td>or equivalent</td></tr><tr><td>Fibronectin coated plates&amp;nbsp;</td><td>BD Bioscience</td><td>354501</td><td>or equivalent</td></tr><tr><td>Fetal bovine serum&amp;nbsp;</td><td>Hyclone</td><td>SH30910.03</td><td>or equivalent</td></tr><tr><td>Heart bioreactor glassware</td><td>Radnoti Glass Technology</td><td>120101BEZ</td><td>Must be sterilizable by autoclaving or gas.</td></tr></tbody></table>

neonatal cardiac scaffolds: novel matrices for regenerative studies

The only definitive therapy for end stage heart failure is orthotopic heart transplantation. Each year, it is estimated that more than 100,000 donor hearts are needed for cardiac transplantation procedures in the United States1-2. Due to the limited numbers of donors, only approximately 2,400 transplants are performed each year in the U.S.2. Numerous approaches, from cell therapy studies to implantation of mechanical assist devices, have been undertaken, either alone or in combination, in an attempt to coax the heart to repair itself or to rest the failing heart3. In spite of these efforts, ventricular assist devices are still largely used for the purpose of bridging to transplantation and the utility of cell therapies, while they hold some curative promise, is still limited to clinical trials. Additionally, direct xenotransplantation has been attempted but success has been limited due to immune rejection. Clearly, another strategy is required to produce additional organs for transplantation and, ideally, these organs would be autologous so as to avoid the complications associated with rejection and lifetime immunosuppression. Decellularization is a process of removing resident cells from tissues to expose the native extracellular matrix (ECM) or scaffold. Perfusion decellularization offers complete preservation of the three dimensional structure of the tissue, while leaving the bulk of the mechanical properties of the tissue intact4. These scaffolds can be utilized for repopulation with healthy cells to generate research models and, possibly, much needed organs for transplantation. We have exposed the scaffolds from neonatal mice (P3), known to retain remarkable cardiac regenerative capabilities,5-8 to detergent mediated decellularization and we repopulated these scaffolds with murine cardiac cells. These studies support the feasibility of engineering a neonatal heart construct. They further allow for the investigation as to whether the ECM of early postnatal hearts may harbor cues that will result in improved recellularization strategies.

Decellularization 
On average, the time to decellularization of a P3 heart using this protocol is approximately 14 hr. given an average heart weight of 23 mg for the P3 neonate.
Acellularity 
Figure 3a demonstrates a fully intact P3 neonatal heart (whole mount). Figure 3b shows the same heart following decellularization. Figures 4a and 4b show the hema...

Watch this Scientific Journal Video about Neonatal Cardiac Scaffolds: Novel Matrices for Regenerative Studies at JoVE.com

Neonatal Cardiac Scaffolds: Novel Matrices for Regenerative Studies

In these studies, we provide methodology for novel, neonatal, murine cardiac scaffolds for use in regenerative studies.

The only definitive therapy for end stage heart failure is orthotopic heart transplantation.  Each year, it is estimated that more than 100,000 donor ...

neonatal-cardiac-scaffolds-novel-matrices-for-regenerative-studies

Research

JoVE Journal

Bioengineering

7.7K Views.  University of Minnesota.  In deze studies geven we nieuwe methodologie voor neonatale muizen cardiale scaffolds voor gebruik in regeneratieve studies. 

Video: Neonatal Cardiac Scaffolds: Novel Matrices for Regenerative Studies

Capillary Force Lithography for Cardiac Tissue Engineering

Cardiovascular disease remains the leading cause of death worldwide1. Cardiac tissue engineering holds much promise to deliver groundbreaking medical discoveries with the aims of developing functional tissues for cardiac regeneration as well as in vitro screening assays. However, the ability to create high-fidelity models of heart tissue has proven difficult. The heart&#8217;s extracellular matrix (ECM) is a complex structure consisting of both biochemical and biomechanical signals ranging from the micro- to the nanometer scale2. Local mechanical loading conditions and cell-ECM interactions have recently been recognized as vital components in cardiac tissue engineering3-5.
A large portion of the cardiac ECM is composed of aligned collagen fibers with nano-scale diameters that significantly influences tissue architecture and electromechanical coupling2. Unfortunately, few methods have been able to mimic the organization of ECM fibers down to the nanometer scale. Recent advancements in nanofabrication techniques, however, have enabled the design and fabrication of scalable scaffolds that mimic the in vivo structural and substrate stiffness cues of the ECM in the heart6-9.
Here we present the development of two reproducible, cost-effective, and scalable nanopatterning processes for the functional alignment of cardiac cells using the biocompatible polymer poly(lactide-co-glycolide) (PLGA)8 and a polyurethane (PU) based polymer. These anisotropically nanofabricated substrata (ANFS) mimic the underlying ECM of well-organized, aligned tissues and can be used to investigate the role of nanotopography on cell morphology and function10-14.
Using a nanopatterned (NP) silicon master as a template, a polyurethane acrylate (PUA) mold is fabricated. This PUA mold is then used to pattern the PU or PLGA hydrogel via UV-assisted or solvent-mediated capillary force lithography (CFL), respectively15,16. Briefly, PU or PLGA pre-polymer is drop dispensed onto a glass coverslip and the PUA mold is placed on top. For UV-assisted CFL, the PU is then exposed to UV radiation (&#955; = 250-400 nm) for curing. For solvent-mediated CFL, the PLGA is embossed using heat (120 &#176;C) and pressure (100 kPa). After curing, the PUA mold is peeled off, leaving behind an ANFS for cell culture. Primary cells, such as neonatal rat ventricular myocytes, as well as human pluripotent stem cell-derived cardiomyocytes, can be maintained on the ANFS2.

In this protocol, we demonstrate the fabrication of biomimetic cardiac cell culture substrata made from two distinct polymeric materials using capillary force lithography. The described methods provide a scalable, cost-effective technique to engineer the structure and function of macroscopic cardiac tissues for in vitro and in vivo applications.

Cardiovascular disease remains the leading cause of death worldwide1. Cardiac tissue engineering holds much promise to deliver groundbreaking medical ...

Tissue Engineering: Construction of a Multicellular 3D Scaffold for the Delivery of Layered Cell Sheets

Many tissues, such as the adult human hearts, are unable to adequately regenerate after damage.2,3 Strategies in tissue engineering propose innovations to assist the body in recovery and repair. For example, TE approaches may be able to attenuate heart remodeling after myocardial infarction (MI) and possibly increase total heart function to a near normal pre-MI level.4 As with any functional tissue, successful regeneration of cardiac tissue involves the proper delivery of multiple cell types with environmental cues favoring integration and survival of the implanted cell/tissue graft. Engineered tissues should address multiple parameters including: soluble signals, cell-to-cell interactions, and matrix materials evaluated as delivery vehicles, their effects on cell survival, material strength, and facilitation of cell-to-tissue organization. Studies employing the direct injection of graft cells only ignore these essential elements.2,5,6 A tissue design combining these ingredients has yet to be developed. Here, we present an example of integrated designs using layering of patterned cell sheets with two distinct types of biological-derived materials containing the target organ cell type and endothelial cells for enhancing new vessels formation in the &#8220;tissue&#8221;. Although these studies focus on the generation of heart-like tissue, this tissue design can be applied to many organs other than heart with minimal design and material changes, and is meant to be an off-the-shelf product for regenerative therapies. The protocol contains five detailed steps. A temperature sensitive Poly(N-isopropylacrylamide) (pNIPAAM) is used to coat tissue culture dishes. Then, tissue specific cells are cultured on the surface of the coated plates/micropattern surfaces to form cell sheets with strong lateral adhesions. Thirdly, a base matrix is created for the tissue by combining porous matrix with neovascular permissive hydrogels and endothelial cells. Finally, the cell sheets are lifted from the pNIPAAM coated dishes and transferred to the base element, making the complete construct.

For creation of highly organized structures of complex tissue, one must assemble multiple material and cell types into an integrated composite. This combinatorial design incorporates organ-specific layered cell sheets with two distinct biologically-derived materials containing a strong fibrous matrix base, and endothelial cells for enhancing new vessels formation.

Many tissues, such as the adult human hearts, are unable to adequately regenerate after damage.2,3 Strategies in tissue engineering propose innovations to ...

Fabrication of Myogenic Engineered Tissue Constructs

Despite the fact that electronic pacemakers are life-saving medical devices, their long-term performance in pediatric patients can be problematic owing to the restrictions imposed by a child's small size and their inevitable growth. Consequently, there is a genuine need for innovative therapies designed specifically for pediatric patients with cardiac rhythm disorders. We propose that a conductive biological alternative consisting of a collagen-based matrix containing autologously-derived cells could better adapt to growth, reduce the need for recurrent surgeries, and greatly improve the quality of life for these patients. In the present study, we describe a procedure for incorporating primary skeletal myoblast cell cultures within a hydrogel matrix to fashion a surgically-implantable tissue construct that will serve as an electrical conduit between the upper and lower chambers of the heart. Ultimately, we anticipate using this type of engineered tissue to restore atrioventricular electrical conduction in children with complete heart block. In view of that, we isolate myoblasts from the skeletal muscles of neonatal Lewis rats and plate them onto laminin-coated tissue culture dishes using a modified version of established protocols[2, 3]. After one to two days, cultured cells are collected and mixed with antibiotics, type 1 collagen, Matrigel&trade;, and NaHCO3. The result is a viscous, uniform solution that can be cast into a mold of nearly any shape and size[1, 4, 5]. For our tissue constructs, we employ type 1 collagen isolated from fetal lamb skin using standard procedures[6]. Once the tissue has solidified at 37&deg;C, culture media is carefully added to the plate until the construct is submerged. The engineered tissue is then allowed to further condense through dehydration for 2 more days, at which point it is ready for in vitro assessment or surgical-implantation.

Here, we demonstrate fabrication of collagen-based, tissue constructs containing skeletal myoblasts. These 3-D engineered constructs may be used to replace or repair tissues in vivo. For our purposes, we have designed these as an atrioventricular electrical conduit for the repair of complete heart block[1].

Despite the fact that electronic pacemakers are life-saving medical devices, their long-term performance in pediatric patients can be problematic owing to ...

Biology

Comparable Decellularization of Fetal and Adult Cardiac Tissue Explants as 3D-like Platforms for In Vitro Studies

Current knowledge of extracellular matrix (ECM)-cell communication translates to large two-dimensional (2D) in vitro culture studies where ECM components are presented as a surface coating. These culture systems constitute a simplification of the complex nature of the tissue ECM that encompasses biochemical composition, structure, and mechanical properties. To better emulate the ECM-cell communication shaping the cardiac microenvironment, we developed a protocol that allows for the decellularization of the whole fetal heart and adult left ventricle tissue explants simultaneously for comparative studies. The protocol combines the use of a hypotonic buffer, a detergent of anionic surfactant properties, and DNase treatment without any requirement for specialized skills or equipment. The application of the same decellularization strategy across tissue samples from subjects of various age is an alternative approach to perform comparative studies. The present protocol allows the identification of unique structural differences across fetal and adult cardiac ECM mesh and biological cellular responses. Furthermore, the herein methodology demonstrates a broader application being successfully applied in other tissues and species with minor adjustments, such as in human intestine biopsies and mouse lung.

The cardiac extracellular matrix (ECM) is a complex network of molecules that orchestrate key processes in tissues and organs while enduring physiological remodeling throughout life. Standardized decellularization of fetal and adult hearts permits comparative experimental studies of both tissues in a 3D context by capturing native architecture and biomechanical properties.

Current knowledge of extracellular matrix (ECM)-cell communication translates to large two-dimensional (2D) in vitro culture studies where ECM components ...

A Net Mold-based Method of Scaffold-free Three-Dimensional Cardiac Tissue Creation

This protocol describes a novel and easy net mold-based method to create three-dimensional (3-D) cardiac tissues without additional scaffold material. Human-induced pluripotent stem-cell-derived cardiomyocytes (iPSC-CMs), human cardiac fibroblasts (HCFs), and human umbilical vein endothelial cells (HUVECs) are isolated and used to generate a cell suspension with 70% iPSC-CMs, 15% HCFs, and 15% HUVECs. They are co-cultured in an ultra-low attachment "hanging drop" system, which contains micropores for condensing hundreds of spheroids at one time. The cells aggregate and spontaneously form beating spheroids after 3 days of co-culture. The spheroids are harvested, seeded into a novel mold cavity, and cultured on a shaker in the incubator. The spheroids become a mature functional tissue approximately 7 days after seeding. The resultant multilayered tissues consist of fused spheroids with satisfactory structural integrity and synchronous beating behavior. This new method has promising potential as a reproducible and cost-effective method to create engineered tissues for the treatment of heart failure in the future.

This protocol describes a net mold-based method to create three-dimensional scaffold-free cardiac tissues with satisfactory structural integrity and synchronous beating behavior.

This protocol describes a novel and easy net mold-based method to create three-dimensional (3-D) cardiac tissues without additional scaffold material. ...

Fabrication of Decellularized Cartilage-derived Matrix Scaffolds

Osteochondral defects lack sufficient intrinsic repair capacity to regenerate functionally sound bone and cartilage tissue. To this extent, cartilage research has focused on the development of regenerative scaffolds. This article describes the development of scaffolds that are completely derived from natural cartilage extracellular matrix, coming from an equine donor. Potential applications of the scaffolds include producing allografts for cartilage repair, serving as a scaffold for osteochondral tissue engineering, and providing in vitro models to study tissue formation. By decellularizing the tissue, the donor cells are removed, but many of the natural bioactive cues are thought to be retained. The main advantage of using such a natural scaffold in comparison to a synthetically produced scaffold is that no further functionalization of polymers is required to drive osteochondral tissue regeneration. The cartilage-derived matrix scaffolds can be used for bone and cartilage tissue regeneration in both in vivo and in vitro settings.

Decellularized cartilage-derived scaffolds can be used as a scaffold to guide cartilage repair and as a means to regenerate osteochondral tissue. This paper describes the decellularization process in detail and provides suggestions to use these scaffolds in in vitro settings.

Osteochondral defects lack sufficient intrinsic repair capacity to regenerate functionally sound bone and cartilage tissue. To this extent, cartilage ...

Preparation of Mesh-Shaped Engineered Cardiac Tissues Derived from Human iPS Cells for In Vivo Myocardial Repair

The current protocol describes methods to generate scalable, mesh-shaped engineered cardiac tissues (ECTs) composed of cardiovascular cells derived from human induced pluripotent stem cells (hiPSCs), which are developed towards the goal of clinical use. HiPSC-derived cardiomyocytes, endothelial cells, and vascular mural cells are mixed with gel matrix and then poured into a polydimethylsiloxane (PDMS) tissue mold with rectangular internal staggered posts. By culture day 14 ECTs mature into a 1.5 cm x 1.5 cm mesh structure with 0.5 mm diameter myofiber bundles. Cardiomyocytes align to the long-axis of each bundle and spontaneously beat synchronously. This approach can be scaled up to a larger (3.0 cm x 3.0 cm) mesh ECT while preserving construct maturation and function. Thus, mesh-shaped ECTs generated from hiPSC-derived cardiac cells may be feasible for cardiac regeneration paradigms.

The present protocol generates mesh-shaped engineered cardiac tissues containing cardiovascular cells derived from human induced pluripotent stem cells to allow the investigation of cell implantation therapy for heart diseases.

The current protocol describes methods to generate scalable, mesh-shaped engineered cardiac tissues (ECTs) composed of cardiovascular cells derived from ...

Generation, High-Throughput Screening, and Biobanking of Human-Induced Pluripotent Stem Cell-Derived Cardiac Spheroids

Human-induced pluripotent stem cell-derived cardiomyocytes (hiPSC-CMs) are of paramount importance for human cardiac disease modeling and therapeutics. We recently published a cost-effective strategy for the massive expansion of hiPSC-CMs in two dimensions (2D). Two major limitations are cell immaturity and a lack of three-dimensional (3D) arrangement and scalability in high-throughput screening (HTS) platforms. To overcome these limitations, the expanded cardiomyocytes form an ideal cell source for the generation of 3D cardiac cell culture and tissue engineering techniques. The latter holds great potential in the cardiovascular field, providing more advanced and physiologically relevant HTS. Here, we describe an HTS-compatible workflow with easy scalability for the generation, maintenance, and optical analysis of cardiac spheroids (CSs) in a 96-well-format. These small CSs are essential to fill the gap present in current in vitro disease models and/or generation for 3D tissue engineering platforms. The CSs present a highly structured morphology, size, and cellular composition. Furthermore, hiPSC-CMs cultured as CSs display increased maturation and several functional features of the human heart, such as spontaneous calcium handling and contractile activity. By automatization of the complete workflow, from the generation of CSs to functional analysis, we increase intra- and inter-batch reproducibility as demonstrated by high-throughput (HT) imaging and calcium handling analysis. The described protocol allows modeling of cardiac diseases and assessing drug/therapeutic effects at the single-cell level within a complex 3D cell environment in a fully automated HTS workflow. In addition, the study describes a straightforward procedure for long-term preservation and biobanking of whole-spheroids, thereby providing researchers the opportunity to create next-generation functional tissue storage. HTS combined with long-term storage will substantially contribute to translational research in a wide range of areas, including drug discovery and testing, regenerative medicine, and the development of personalized therapies.

Presented here is a set of protocols for the generation and cryopreservation of cardiac spheroids (CSs) from human-induced pluripotent stem cell-derived cardiomyocytes cultured in a high-throughput, multidimensional format. This three-dimensional model functions as a robust platform for disease modeling, high-throughput screenings, and maintains its functionality after cryopreservation.

Human-induced pluripotent stem cell-derived cardiomyocytes (hiPSC-CMs) are of paramount importance for human cardiac disease modeling and therapeutics. We ...

3D Human Myocardial Tissue Generation Using Melt Electrospinning Writing of Polycaprolactone Scaffolds and hiPSC-Derived Cardiac Cells

The development of functional human cardiac tissues holds significant promise for advancing applications in drug screening, disease modeling, and regenerative medicine. This protocol describes the stepwise fabrication of 3D myocardial tissues with advanced mimicry of native cardiac structure by combining melt electrospinning writing (MEW) polycaprolactone (PCL) scaffolds with fibrin hydrogels and human induced pluripotent stem cell (hiPSC)-derived cardiac cells. The process involves embedding a mixture of cardiomyocytes (hiPSC-CMs) and cardiac fibroblasts (hiPSC-CFs) within a fibrin matrix to create mini-tissues, with structural support provided by MEW-generated scaffolds. These fibrillar scaffolds are fabricated at the micro- to nanoscale, allowing for precise control over fiber architecture, which plays a key role in organizing cell distribution and alignment. Meanwhile, the fibrin matrix promotes cell viability and mimics the extracellular environment. Characterization of the generated tissues reveals well-organized sarcomeres within hiPSC-CMs, along with stable contractile activity. The tissues demonstrate consistent spontaneous beating as early as two days post-seeding, with sustained functionality over time. The combination of hiPSC-CFs with hiPSC-CMs enhances the structural integrity of the tissues while supporting long-term cell viability. This approach offers a reproducible, adaptable, and scalable method for creating biomimetic cardiac tissue models, providing a versatile platform for preclinical drug testing, mechanistic studies of cardiac disease, and potential regenerative therapies.

A reproducible method is presented to generate 3D myocardial tissues combining melt electrospinning writing (MEW) polycaprolactone (PCL) scaffolds and fibrin hydrogels with hiPSC-derived cardiomyocytes and fibroblasts. This technique offers precise control over scaffold architecture and can be applied in preclinical drug testing and cardiac disease modeling.

The development of functional human cardiac tissues holds significant promise for advancing applications in drug screening, disease modeling, and ...

In Vivo Heart Transplantation to Study Endothelial-to-Mesenchymal Transition

A Neonatal Heterotopic Rat Heart Transplantation Model for the Study of Endothelial-to-Mesenchymal Transition

Endocardial fibroelastosis (EFE), defined by subendocardial tissue accumulation, has major impacts on the development of the left ventricle (LV) and precludes patients with congenital critical aortic stenosis and hypoplastic left heart syndrome (HLHS) from curative anatomical biventricular surgical repair. Surgical resection is currently the only available therapeutic option, but EFE often recurs, sometimes with an even more infiltrative growth pattern into the adjacent myocardium.
To better understand the underlying mechanisms of EFE and to explore therapeutic strategies, an animal model suitable for preclinical testing was developed. The animal model takes into consideration that EFE is a disease of the immature heart and is associated with flow disturbances, as supported by clinical observations. Thus, the heterotopic heart transplantation of neonatal rat donor hearts is the basis for this model.
A neonatal rat heart is transplanted into an adolescent rat&#39;s abdomen and connected to the recipient&#39;s infrarenal aorta and inferior vena cava. While perfusion of the coronary arteries preserves the viability of the donor heart, flow stagnation within the LV induces EFE growth in the very immature heart. The underlying mechanism of EFE formation is the transition of endocardial endothelial cells to mesenchymal cells (EndMT), which is a well-described mechanism of early embryonic development of the valves and septa but also the leading cause of fibrosis in heart failure. EFE formation can be macroscopically observed within days after transplantation. Transabdominal echocardiography is used to monitor the graft viability, contractility, and the patency of the anastomoses. Following euthanasia, the EFE tissue is harvested, and it shows the same histopathological characteristics as human EFE tissue from HLHS patients.
This in vivo model allows for studying the mechanisms of EFE development in the heart and testing treatment options to prevent this pathological tissue formation and provides the opportunity for a more generalized examination of EndMT-induced fibrosis.

Author Spotlight: A Neonatal Heterotopic Rat Heart Transplantation Model for the Study of Endothelial-to-Mesenchymal Transition  

This work presents an animal model of endothelial-to-mesenchymal transition-induced fibrosis, as seen in congenital cardiac defects such as critical aortic stenosis or hypoplastic left heart syndrome, which allows for detailed histological tissue evaluation, the identification of regulatory signaling pathways, and the testing of treatment options.

Endocardial fibroelastosis (EFE), defined by subendocardial tissue accumulation, has major impacts on the development of the left ventricle (LV) and ...

Neonatal Cardiac Scaffolds: Novel Matrices for Regenerative Studies

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