This work was supported by Charles University research grants GA UK No. 538216 and GA UK No. 1114213.

This experimental protocol was reviewed and approved by the Institutional Animal Expert Committee at First Faculty of Medicine, Charles University, and was performed at the University experimental laboratory, Department of Physiology, First Faculty of Medicine, Charles University in Prague, Czech Republic, in accordance with Act No. 246/1992 Coll., on the protection of animals against cruelty. All animals were treated and cared for in accordance with the Guide for the Care and Use of Laboratory Animals, 8th edition, published by National Academies Press, 2011. All procedures were performed according to standard veterinary conventions and at the completion of each study, the animal was sacrificed and a necropsy performed. Due to suitable anatomy, five healthy crossbred female swine (Sus scrofa domestica) up to 6 months of age were included in this experiment. Their mean body weight was 66 &#177; 20 kg at the day of data collection.
1. General Anesthesia
<ol>
	<li>After 1 day of fasting, initiate anesthesia by intramuscular administration of midazolam (0.3 mg/kg) and ketamine hydrochloride (15 - 20 mg/kg) to the gluteal region.</li>
	<li>Insert peripheral cannula into the marginal ear vein for intravenous drug applications.</li>
	<li>Administer intravenous boluses of propofol (2 mg/kg) and morphine (0.1 - 0.2 mg/kg).</li>
	<li>Provide animals with oxygen via a facial mask and advance orotracheal intubation with a cuffed endotracheal tube with a diameter of 6.5 - 7.5 mm.</li>
	<li>Continue the total intravenous anesthesia by combination of propofol (6 - 12 mg/kg/h), midazolam (0.1 - 0.2 mg/kg/h), and morphine (0.1 - 0.2 mg/kg/h), adjusting the doses according to individual responses - suppress spontaneous breaths, corneal reflexes, and motoric response. Protect the animal&#39;s eyes with ointment to prevent dryness.</li>
	<li>Operate the mechanical ventilation by a closed-loop automatic device set to adaptive support ventilation to maintain target end-tidal CO2 of 38 - 42 mmHg and adequate hemoglobin saturation of 95 - 99%. Monitor all vital functions, especially heart rate and body temperature.</li>
	<li>Attach the animal by securing its legs gently to the operation table in the supine position.</li>
	<li>Administer wide spectrum antibiotics - 1 g of cefazolin intravenously through the ear vein cannula.</li>
</ol>
2. Ventricular Lead Implantation
<ol>
	<li>Locate surgical sites and shave the skin properly using a razor at (1) the jugular region above the sternocleidomastoid muscle and (2) the unilateral paravertebral region on the back side of the animal&#39;s neck.</li>
	<li>Using the ultrasound vascular probe, visualize the external jugular vein and mark its location on the skin. Locate the carotid artery as well to prevent its injury.</li>
	<li>After the wide skin disinfection using povidone iodine, cover with a sterile surgical drape with the hole over the marked jugular region.</li>
	<li>Prepare all necessary tools for pacemaker implantation and keep them sterile. It is crucial to maintain a sterile environment throughout the procedure.</li>
	<li>Cut the skin parallel above the external jugular vein, form a shallow subcutaneous pocket in soft tissue not more than 10 mm deep. Do not expose any large vessels.</li>
	<li>From the bottom of the preformed pocket, insert a sheath into the external jugular vein, using the standard Seldinger technique. First, insert a soft-tip guidewire through a 12G puncture needle, and then over the guidewire introduce a 7-French plastic tear away introducer sheath with a dilator.</li>
	<li>Under fluoroscopic guidance, introduce a 58 cm pacing lead through this sheath and position its tip to the apex of the right ventricle. Then, remove the sheath and fixate the active tip of the electrode to the myocardium by screwing out its helix.</li>
	<li>Test the pacing parameters - the lead sensed signal from ventricular electrocardiogram and impedance must be stable, the pacing threshold should be below an amplitude of 1 V with 0.4 ms of pulse duration.</li>
	<li>Pull a rubber sleeve on the pacing lead and fix both together to the bottom of the preformed jugular subcutaneous pocket by two non-absorbable suture braided thread stitches. Importantly, enough length of the pacing lead must be inserted, considering the future possible growth of the animal.</li>
</ol>
3. Subcutaneous Lead Tunneling
<ol>
	<li>Turn the animal over on its side and disinfect the previously shaved skin region lateral to the backbone, then cover with a sterile surgical drape with a hole. Make sure the jugular subcutaneous pocket and the lead remain sterile.</li>
	<li>Cut the skin lateral to the backbone and form a deep, spacious, subcutaneous pocket. Use dull preparation and stop any possible bleeding.</li>
	<li>Take a soft rubber extension tube from a sterile infusion set and cut off both its ends. Using a tunneling tool, preform a direct subcutaneous tunnel connecting the jugular and dorsal subcutaneous pockets with this extension tube.</li>
	<li>Connect the tube&#39;s free end to the ventricular lead by pulling it onto its IS-1 connector and draw the lead through the preformed tunnel into the dorsal subcutaneous pocket by pulling the tube dorsally. It may be useful to secure the connection with a silk tie.</li>
	<li>Remove both the tunneling tool and the extension tube, exposing the ventricular lead from the dorsal subcutaneous pocket.</li>
</ol>
4. Pacemaker Implantation
<ol>
	<li>Set up the implantable dual-chamber heart pacemaker unit with the &#34;Y&#34; connecting part. The &#34;Y&#34; connection allows a convergent connection of both pacemaker outputs to be joined and connected together to the single pacing lead (Figure 1 and Figure 2). This setting will later provide a wide range of pacing frequencies.</li>
	<li>After connecting the pacing lead, fasten all the IS-1 connection screws in the pacemaker header unit and the &#34;Y&#34; lead connection.</li>
	<li>Hide the whole pacing system in the deep dorsal pocket. There must be enough space to comfortably accommodate the pacemaker unit and any redundant lead.</li>
	<li>Check the final pacing parameters. Make sure that cardiac ventricular pacing is possible from both pacemaker outputs.</li>
	<li>Flush with povidone iodine and close both subcutaneous pockets. Use absorbable braided thread to suture fibrous tissue layers and non-absorbable suture for skin adaptation.</li>
</ol>
5. Postoperative Care
<ol>
	<li>Observe the animal carefully until it regains sufficient consciousness.</li>
	<li>Continue in a wide spectrum intravenous antibiotic regimen until the wounds are healed - cefazolin 1 g every 12 h. Administer analgesics in appropriate dosing, e.g., morphine 0.2 mg/kg every 6 - 12 h for 3 days by subcutaneous injection. If necessary, make dose adjustments to adequately prevent pain.</li>
	<li>Place the animal in a comfortable, calm facility at room temperature. Allow free access to water and suitable alimentation.</li>
	<li>Dress the wounds with sterile scrubs regularly to preserve clean healing.</li>
	<li>To provide rest after the surgical procedure, keep the pacemaker inhibited by native heart rhythm&#160;for at least 3 days.</li>
	<li>Remove the non-absorbable skin sutures when fully healed, approximately 10 - 14 days after the procedure.</li>
</ol>
6. Pacing Protocol
<ol>
	<li>Start the pacing protocol after an adequate resting period. Initially, increase the paced ventricular heart rate to 200 beats/min by setting the dual-chamber pacemaker to mode D00, 100 beats/min, and concomitantly adjusting the AV delay to 300 ms (to exactly match the pace to pace interval, see Table 1). Select the unipolar pacing in both outputs.</li>
	<li>Increase stepwise the paced heart rate to 220 beats/min after 1 week and to 240 beats/min after 2 weeks (Figure 3). Keep continuous pacing at this frequency unless it is not hemodynamically tolerated. If the HF progresses too quickly, reduce the paced heart rate before increasing it again after another week.</li>
	<li>Use auscultation of heart beat, ECG, and pacemaker interrogation daily to verify the heart rate and constant pacing parameters, including battery life.</li>
</ol>
7. Heart Failure Induction and Monitoring
<ol>
	<li>Ensure regular care by a specialized veterinarian and monitor the animal&#39;s general health status. Clinical observations of increasing native heart and respiratory rates, evaluation of peripheral pulse oximetry, and reduction in spontaneous physical activity or appetite provide information about HF progression.</li>
	<li>Use the advantage of wireless transcutaneous pacemaker interrogation and, if possible, continuous ECG recording - frequent non-sustained ventricular tachycardias (VT) are a sign of severe HF progression.</li>
	<li>Use echocardiographic assessments to reveal the structural and functional heart changes. Pay attention to find an optimal image window according to porcine anatomy and heart dilation - for a typical 4 chamber view, place the transducer to the right just below the xiphoid and angle it to point to the neck or left shoulder. For short-axis views, use intercostal windows. Reduction of ventricular ejection fraction in native heart rhythm and atrioventricular regurgitations should be noticeable after a few weeks. 
	NOTE: Significant interindividual differences of high rate ventricular pacing tolerance exist. Therefore, frequent monitoring and individually adapted adjustment of the pacing protocol are necessary.</li>
</ol>
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/57030/57030fig1.jpg" /> 
Figure 1: Heart pacing unit schematic. The dual-chamber pacemaker (1), a &#34;Y&#34; shaped adapter (2) conducting convergently both pacemaker outputs together to a single pacing lead (3). The tip of the lead is fixated into the apical part of the RV cavity (4). This setting provides a wide range of high pacing frequencies. <a href="//cloudfront-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57030/57030fig1large.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/57030/57030fig2.jpg" /> 
Figure 2: Heart pacing unit. X-ray&#160;(A) and photography (B) of the dual-chamber pacemaker (1), a &#34;Y&#34; shaped adapter (2), and the ventricular pacing lead (3). <a href="//cloudfront-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57030/57030fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Desired HR</td>
			<td>Set pacemaker rate</td>
			<td>Pace to pace interval</td>
		</tr>
		<tr>
			<td>beats/min</td>
			<td>beats/min</td>
			<td>ms</td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>200</td>
			<td>100</td>
			<td>300</td>
		</tr>
		<tr>
			<td>220</td>
			<td>110</td>
			<td>270</td>
		</tr>
		<tr>
			<td>240</td>
			<td>120</td>
			<td>250</td>
		</tr>
		<tr>
			<td>250</td>
			<td>125</td>
			<td>240</td>
		</tr>
	</tbody>
</table>
Table 1: Pacemaker parameters. To allow high rate cardiac pacing with the implanted in-house-modified dual-chamber pacemaker unit, the table shows the desired paced heart rate (HR) and matching pace to pace interval values. The pacemaker must be set to D00 operation mode at a rate of half of the desired HR, and the AV delay set to the corresponding pace to pace interval in milliseconds.
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/57030/57030fig3.jpg" /> 
Figure 3: Pacing protocol. The progressive phase of the TIC induction starts after a resting period of 3 days. Then, the pacemaker is set to D00 mode with a pacing frequency of 50% of the desired paced frequency, and AV delay is set to the matching pace to pace interval (see Table 1). Thanks to the &#34;Y&#34; shaped adapter, both pacemaker outputs are conducted to a single pacing lead. bpm = beats/minute. <a href="//cloudfront-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57030/57030fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

The authors have nothing to disclose.

Chronic HF is a major health problem that contributes greatly to morbidity and mortality. The pathogenesis and progression of HF in humans is complex, so an appropriate animal model is critical to investigate the underlying mechanisms and to test novel therapeutics that aim to interfere with native severe disease progression. To study its pathogenesis, large animal models are being used for experimental testing.
In general, surgical models of chronic HF closely mimic this disease. When compared to models of acute HF, chronic HF models offer more insight into the pathophysiology, but at the cost of time consuming experimental preparation or higher mortality rate. From the variety of known chronic HF models, we are referring to an appropriate and easily manageable model, represented here by decompensated chronic HF induced by paced tachycardia.
Tachycardia-induced cardiomyopathy as a form of dilated cardiomyopathy is inducible by fast cardiac pacing. The pacing electrode can be located in the ventricles or atria19,24. We omitted the supraventricular pacing site to prevent problems possibly caused by atrioventricular block during high pacing frequencies. The ventricular position also improved the stability of the pacing lead fixated in the ventricular apex compared to the atrial position and reduced occurrence of its dislocation. The presented methodology is specifically designed for easy performance, use of widely available equipment, and prevention of complications. Another goal of this method was to easily control chronic HF progression by titration of the pacing protocol.
Bacterial infection complications are a major problem of implants in experimental settings. Generator pocket infections and infective endocarditis are both associated with poor prognoses and would make the experiment futile. Due to porcine anatomy, the jugular region is exposed and if a pacemaker generator was placed here, healing and preventing contamination would be a difficult task in long-survival experiments. The usage of subcutaneous tunneling enables the location of the pacemaker generator pocket to the dorsal region, which is accessible and can be kept in a hygienic state. The pacemaker is also not within the animal&#39;s reach, which considerably improves healing. An alternative approach could be the use of an extracorporeal pacemaker generator attached to the skin surface, but this tactic was shown to be mechanically vulnerable, if long-term animal survival was intended.
All equipment necessary for the described protocol are widely available, and this method is reproducible with basic surgical and catheterization skills. The purpose of the &#34;Y&#34; shaped connection unit is to use a regular dual-chamber pacemaker, as it converges both of its outputs (atrial and ventricular) to the tip of the single pacing lead. These settings allow a wide range of high rate pacing frequencies (200 - 300 beats/min, Figure 1 and Table 1).
The most critical step is the titration of pacing frequencies. Too high from the beginning would cause acute decompensation with no time for the adaptation mechanisms to develop; conversely, titrating the pacing too low would be well tolerated and would prolong the HF induction.
According to previous publications22,25,37 and the authors&#39; experience, the pacing protocol was defined and started with pacing rate of 200 beats/min, which is above physiological rate of healthy swine in exercise or stress. Subsequently, the frequency was escalated and titrated between 200 and 240 beats/min with respect to individual HF progression13,19. Due to interindividual differences in response to fast pacing, the time needed to produce chronic HF with profound signs of decompensation varied from 4 to 8 weeks. An issue here can become the battery life, as such high rate pacing increases energy demands. Especially when the pacing threshold is elevated, regular interrogations are important.
After the pacing protocol, symptoms of chronic HF were prominent consistently in all animals - tachypnea, fatigue, spontaneous tachycardia of &#62;150 beats/min, and systolic murmurs. After further clinical investigation, ascites, pericardial and pleural effusions, non-sustained ventricular tachycardias, dilation of all heart chambers, and significant mitral and tricuspid regurgitations were described. Failing hemodynamics was indicated by arterial hypotension, poor myocardial contractility, low stroke volume, and cardiac output reduced to approximately 50% of a healthy animal&#39;s expected normal value38. This developed model of tachycardia induced cardiomyopathy matched well to poorly compensated dilated cardiomyopathy and was also preserved after the cessation of pacing21,39,40.
The fact that systolic function continues to be severely deteriorated after cessation of pacing makes the model an excellent choice to examine HF in native sinus rhythm. It has been previously shown that tachycardia-induced systolic dysfunction is at least partially reversible in the so-called recovery phase, but the time needed for it to improve or normalize varies significantly between individuals. The pacing protocol duration and aggressiveness of rate titration may be a significant contributor too, as permanent ischemic and fibrotic changes are produced in the myocardium22,39,40,41. The persistence of severe systolic dysfunction in the presented model was tested at least for 12 h after the pacing had been ceased4 and the qualities of the prepared model including neurohumoral dynamics, peripheral vascular abnormalities, and cardiac dysfunction were reflective of human chronic HF14.
The presented results demonstrate severely deteriorated hemodynamics, both clinical investigation and measured values indicate induction of HF syndrome. Cardiomegaly was consistently observed by clinical examination, imaging, and autopsy. Heart rate of sinus rhythm after the cessation of fast pacing was elevated from normal resting frequency, but we assume that the influence of cardiodepressive effects of anesthetics could limit this spontaneous tachycardia. Aortic pressures show deep hypotension42 and CVP was elevated.
Functional reflection is then the failing circulation and tissue hypoperfusion. These are primarily caused by impaired myocardial contraction, as indicated by the low ejection fraction of the left ventricle. Both ventricles were dilated with no extension in wall thickness, and this heart remodeling was grounds for progressive atrioventricular regurgitations and consequently low cardiac output. As no anatomical shunts were found postmortem, the cardiac output was equally low in systemic as well as in pulmonary circulation, and so the thermodilution derived cardiac output measurements in the pulmonary artery were used to calibrate the PV loop volume characteristics.
The brachial and brain regional tissue oxygen saturation as well as the regional blood flow in subclavian and carotid artery suggests centralization of the blood circulation. Their low values show severely reduced tissue perfusion in peripheral as well as in vital organs, which was confirmed by low SvO2 when compared to the expected normal value of at least 65%42. The general low tissue perfusion was in concordance with the measurements of low cardiac output.
Hemodynamics and mechanical work during each cardiac cycle of the left ventricle was well documented by the PV diagram obtained from PV catheter instant measurements. Poor myocardial strength was denoted by maximum LV peak pressure during systole and the dP/dtmax / EDV ratio, a preload independent index of LV contractility. LV chamber volumes were enlarged during the whole cycle, thus the image of dilated cardiomyopathy. The end-diastolic LV pressure was not increased as high as would be expected in cardiogenic shock. The LV filling pressure remains low, most likely due to high compliance of the LV thin myocardial wall43.
In the vast majority of previous TIC studies, porcine and canine models have been used19. However, rapid pacing can be used to induce cardiomyopathy in other species, even in small animals. Few studies have demonstrated metabolic effects of acute TIC in rats44 or myocardial contractility impairment after long-term fast pacing in rabbits45.
Although this model is adequately reliable, it has several limitations. Non-sustained ventricular tachycardias are a sign of successful HF induction, but long-lasting VT produce risks of sudden cardiac death. During anesthesia, one of the animals required resuscitation and defibrillation. The wide dispersion of results was partly due to differences in animal body weight. Also, the necessity of anesthesia has to be taken under consideration when reporting the results, especially its influence on heart rate and blood pressure. Blood levels of porcine-specific markers could be useful for assessment of the degree of cardiac remodeling, but the evidence on this front is still lacking. As most of these measurement methods were invasive and thus unrepeatable, we did not provide a baseline or sham subject measurement.
A model of progressive chronic heart failure can be produced by the presented methodology. This technique is easy to perform with widely available equipment, and the results are robust and reproducible. This tachycardia-induced cardiomyopathy offers a valuable object for further experimental studies on hemodynamics, investigation of disease mechanisms and effects of applied treatments.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>positives</td>
			<td>negatives</td>
		</tr>
		<tr>
			<td>chronic heart failure syndrome with systemic adaptation</td>
			<td>time consuming model preparation</td>
		</tr>
		<tr>
			<td>easy control of disease progression</td>
			<td>close monitoring necessary</td>
		</tr>
		<tr>
			<td>lead tunneling prevents infective complications</td>
			<td>risk of lead dislocation</td>
		</tr>
		<tr>
			<td>done with basic surgical and cathetrization skills</td>
			<td>risk of malignant arrhythmia</td>
		</tr>
		<tr>
			<td>potentially transferable to different animal species</td>
			<td></td>
		</tr>
	</tbody>
</table>
Table 3: Overview summarizing the positives and negatives of the presented methodology for tachycardia-induced cardiomyopathy in swine as a model of chronic heart failure.

The variety of new treatment methods for heart failure (HF), especially the growing worldwide use of mechanical circulatory supports and extracorporeal membrane oxygenation (ECMO) in clinical practice, is reflecting in preclinical experimental testing. The main focus has been on hemodynamic changes caused by the examined treatment modalities, namely on systemic blood pressure1, myocardial contractility, pressure and volume changes in heart chambers and heart work2,3, arterial blood flow in systemic and peripheral arteries, along with metabolic compensation4 - regional tissue saturation, pulmonary perfusion, and blood gas analysis. Other studies are directed on long-term effects of the circulatory support5, concomitant inflammation, or occurrence of hemolysis. All these types of study need a stable biomodel of congestive HF.
Most of the published experiments on left ventricular (LV) performance and hemodynamics of mechanical circulatory support have been performed on experimental models of acute HF2,6,7,8,9,10, or even on completely intact hearts. On the other hand, in clinical practice, mechanical circulatory supports are often being applied in a status of circulatory decompensation that develops on the grounds of previously present chronic heart disease. In such situations, the adaptation mechanisms are fully developed and can play important roles in inconsistency of outcomes observed according to the &#34;acuteness or chronicity&#34; of underlying cardiac disease11. Therefore, a stable model of chronic HF can offer new insights into pathophysiological mechanisms and hemodynamics. Although there are reasons why the use of chronic HF models is scarce - time consuming preparation, instability of heart rhythm, ethical questions, and mortality rate - their advantages are clear, as they offer presence of long-term neurohumoral activation, general systemic adaptation, functional changes of cardiomyocytes, and structural alterations of heart muscle and valves12,13.
In general, the availability and variety of animal models used for hemodynamic studies is wide and offers choice for many specific needs. For these experiments, mostly porcine, canine, ovine, or with smaller settings murine models, are being chosen and offer a good simulation of expected human bodily reactions14. Furthermore, forms of single organ experiments are becoming more frequent15. To reliably mimic the pathophysiology of HF, circulation is being artificially deteriorated. Damage to the heart can be caused by various methods, often by either ischemia, arrhythmia, pressure overload, or cardiotoxic effects of drugs, with any of these leading to hemodynamic deterioration of the model. To produce a true model of chronic HF, time has to be provided for developing the long-term adaptation of the whole organism. Such a reliable and stable model is represented well by tachycardia-induced cardiomyopathy (TIC), which can be produced by rapid cardiac pacing in experimental animals.
It has been shown that in predisposed hearts, long-lasting incessant tachyarrhythmias can lead to systolic dysfunction and dilation with decreased cardiac output. The condition referred to as TIC was first described in 191316, widely used in experiments since 196217, and is now a well-recognized disorder. Its origin can lie in various types of arrhythmias - both supraventricular and ventricular tachycardia can lead to progressive deterioration of systolic function, biventricular dilation, and progressive clinical signs of HF including ascites, edemas, lethargy, and ultimately cardiac decompensation leading to terminal HF and, if not treated, death.
Similar effects of circulatory suppression were observed by introduction of high rate cardiac pacing in animal models. In a porcine model, an atrial or ventricular heart rate over 200 beats/minute is potent enough to induce end-stage HF in a period of 3 - 5 weeks (progressive phase) with characteristics of TIC, though interindividual differences do exist18,19. These findings correspond well to decompensated cardiomyopathy and are, importantly, preserved also after the cessation of pacing (chronic phase)19,20,21,22,23.
Porcine, canine, or ovine TIC models were repeatedly prepared to study the pathophysiology of HF14, as changes to the LV mimic the characteristics of dilated cardiomyopathy24. The hemodynamic characteristics are well described - increased ventricular end-diastolic pressures, decreased cardiac output, increased systemic vascular resistance, and dilation of both ventricles. In contrast, wall hypertrophy is not observed consistently, and even wall thinning was described by some researchers25,26. With progression of ventricular dimensions, regurgitation on atrioventricular valves develops26.
In this publication, we present a protocol to produce a TIC by long-term fast cardiac pacing in swine. This biomodel represents potent means to study decompensated dilated cardiomyopathy, hemodynamics of progressive chronic HF with low cardiac output, and effects of applied treatment.

<table><tbody><tr><td>&lt;strong&gt;Medication&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>midazolam</td><td>Roche</td><td>Dormicum</td><td>anesthetic</td></tr><tr><td>ketamine hydrochloride</td><td>Richter Gedeon</td><td>Calypsol</td><td>anesthetic</td></tr><tr><td>propofol</td><td>B.Braun</td><td>Propofol</td><td>anesthetic</td></tr><tr><td>cefazolin</td><td>Medochemie</td><td>Azepo</td><td>antibiotic</td></tr><tr><td>Silver Aluminium Aerosol</td><td>Henry Schein</td><td>9003273</td><td>tincture</td></tr><tr><td>povidone iodine</td><td>Egis Praha</td><td>Betadine</td><td>disinfection</td></tr><tr><td>morphine</td><td>Biotika Bohemia</td><td>Morphin 1% inj</td><td>analgetic</td></tr><tr><td>&lt;strong&gt;Tools&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>Metzenbaum scissors, lancet with #22 blade, DeBakey forceps, needle driver</td><td>basic surgical equipment</td><td></td><td></td></tr><tr><td>cauterizer</td><td></td><td></td><td></td></tr><tr><td>2-0 Vicryl</td><td>Ethicon</td><td>V323H</td><td>absorbable braided suture</td></tr><tr><td>2-0 Perma-Hand Silk</td><td>Ethicon</td><td>A185H</td><td>silk tie suture</td></tr><tr><td>2-0 Prolene</td><td>Ethicon</td><td>8433H</td><td>non-absorbable suture</td></tr><tr><td>&lt;strong&gt;Diagnostic devices&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>ESP C-arm</td><td>GE Healthcare</td><td>ESP</td><td>X-ray fluoro C-arm</td></tr><tr><td>Acuson x300</td><td>Siemens Healthcare</td><td></td><td>ultrasound system</td></tr><tr><td>Acuson P5-1</td><td>Siemens Healthcare</td><td></td><td>echocardiographic probe</td></tr><tr><td>Acuson VF10-5</td><td>Siemens Healthcare</td><td></td><td>sonographic vascular probe</td></tr><tr><td>3PSB, 4PSB and 6PSB</td><td>Transonic Systems</td><td></td><td>perivascular flow probes</td></tr><tr><td>TS420</td><td>Transonic Systems</td><td></td><td>perivascular flow module</td></tr><tr><td>TruWave&amp;nbsp;</td><td>Edwards Lifesciences</td><td>T001660A</td><td>fluid-filled pressure transducer</td></tr><tr><td>7.0F VSL Pigtail</td><td>Transonic Systems</td><td></td><td>pressure sensor catheter</td></tr><tr><td>INVOS 5100C Cerebral/Somatic Oximeter</td><td>Somanetics/Medtronic</td><td></td><td>near infrared spectroscopy</td></tr><tr><td>CCO Combo Catheter</td><td>Edwards Lifesciences</td><td>744F75</td><td>Swan-Ganz pulmonary artery catheter</td></tr><tr><td>Vigillace II</td><td>Edwards Lifesciences</td><td>VIG2E</td><td>cardiac output monitor</td></tr><tr><td>7.0F VSL Pigtail</td><td>Transonic Systems</td><td></td><td>pressure-volume catheter</td></tr><tr><td>ADV500</td><td>Transonic Systems</td><td></td><td>pressure-volume system</td></tr><tr><td>LabChart and PowerLab</td><td>ADInstruments</td><td></td><td>data acquisition and analysis system</td></tr><tr><td>Prism 6</td><td>GraphPad</td><td></td><td>statistical analysis software</td></tr><tr><td>&lt;strong&gt;Pacing devices&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>ICS 3000</td><td>Biotronic</td><td>349528</td><td>pacemaker programmer</td></tr><tr><td>ERA 3000</td><td>Biotronic</td><td>128828</td><td>external pacemaker</td></tr><tr><td>Effecta DR</td><td>Biotronic</td><td>371199</td><td>dual-chamber pacemaker</td></tr><tr><td>Tendril STS</td><td>St. Jude Medical</td><td>2088TC/58</td><td>ventricular pacing lead</td></tr><tr><td>Lead permanent adapter</td><td>Osypka</td><td>Article 53422</td><td>convergent &quot;Y&quot; connecting part</td></tr><tr><td>Lead permanent adapter</td><td>Osypka</td><td>Article 53904</td><td>convergent &quot;Y&quot; connecting part</td></tr><tr><td>Tear-Away Introducer 7F</td><td>B.Braun</td><td>5210593</td><td>tear away introducer sheath&amp;nbsp;</td></tr><tr><td>Split Cath Tunneler</td><td>medComp</td><td>AST-L</td><td>tunneling tool</td></tr><tr><td>infusion line</td><td>MPH Medical Devices</td><td>2200045</td><td>connecting line</td></tr></tbody></table>

tachycardia-induced cardiomyopathy as a chronic heart failure model in swine

A stable and reliable model of chronic heart failure is required for many experiments to understand hemodynamics or to test effects of new treatment methods. Here, we present such a model by tachycardia-induced cardiomyopathy, which can be produced by rapid cardiac pacing in swine.
A single pacing lead is introduced transvenously into fully anaesthetized healthy swine, to the apex of the right ventricle, and fixated. Its other end is then tunneled dorsally to the paravertebral region. There, it is connected to an in-house modified heart pacemaker unit that is then implanted in a subcutaneous pocket. 
After 4 - 8 weeks of rapid ventricular pacing at rates of 200 - 240 beats/min, physical examination revealed signs of severe heart failure - tachypnea, spontaneous sinus tachycardia, and fatigue. Echocardiography and X-ray showed dilation of all heart chambers, effusions, and severe systolic dysfunction. These findings correspond well to decompensated dilated cardiomyopathy and are also preserved after the cessation of pacing.
This model of tachycardia-induced cardiomyopathy can be used for studying the pathophysiology of progressive chronic heart failure, especially hemodynamic changes caused by new treatment modalities like mechanical circulatory supports. This methodology is easy to perform and the results are robust and reproducible.

Testing the model: After signs of decompensated chronic HF became prominent, anesthesia and artificial ventilation were administered again following the principles described above, but dosing was adjusted due to low cardiac output27. Due to possible cardiodepressive effects of anesthetics, careful intensive monitoring of vital functions is necessary.
The animal was attached in the supine position and all invasive approaches commenced. The femoral vein and artery and jugular vein were punctured and intravascular approaches ensured by standard percutaneous intraluminal sheaths. Right carotid and subclavian arteries were surgically exposed and circumjacent ultrasound flow probes of appropriate sizes were attached, enabling the obtainment of continuous blood flow measurements28.
Central venous pressure (CVP) was measured via the jugular vein using a standard invasive method with a fluid-filled pressure transducer, but a high-sensitivity pressure sensor equipped catheter in the thoracic aorta was used for systemic arterial pressure measurements. Regional tissue oxygenation was monitored by near-infrared spectroscopy with sensors placed on the head and right forearm representing the brain and peripheral tissue oxygen saturation levels (rSO2)29. A transthoracic echocardiographic probe was used for 2D and color Doppler imaging. Data from ECG, heart rate, pulse oximetry, blood pressures, capnometry, and rectal temperature were centralized on a bed-side monitor for immediate control. A balloon Swan-Ganz catheter was introduced through a femoral vein sheath to the pulmonary artery allowing readings of thermodilution derived continuous cardiac output (CO)30 and mixed venous hemoglobin saturation (SvO2). Through the aortic valve, a pressure-volume (PV) catheter was introduced retrogradely to the LV cavity. This PV conductance catheter enabled the registration of instant volume and pressure in the LV chamber31,32,33,34, and its stable position was guided by fluoroscopy and echocardiography to obtain optimal PV loop morphology (Figure 4 and Figure 5). Measured LV parameters included end-diastolic pressure and volume (EDP and EDV), end-systolic volume (ESV), LV peak pressure (LV PP), and maximal positive change of LV pressure, defined as the first time derivative of LV pressure normalized to EDV (dP/dtmax / EDV), which then represents a preload independent index of LV contractility35,36. Additional calculated parameters were stroke volume (SV = EDV - ESV), left ventricular ejection fraction (EF = SV / EDV), and averaged arterial flow in the carotid and subclavian arteries. Fluoroscopic guidance and X-ray imaging were conducted by a C-arm throughout the protocol. After conclusion of the experimental measurements, euthanasia by intravenous potassium overdose and autopsy were performed. The heart was exposed, cut out from the chest, emptied of blood, weighed, and investigated for structural abnormalities.
All data were acquired in native sinus rhythm after the rapid ventricular pacing had been stopped abruptly and time had been provided for stabilization to steady state conditions. Parameters were then recorded and sets of data averaged from three end-expiratory time points. If present, premature beats were omitted from the analyses. All values are expressed as mean &#177; standard deviation.
Measured results:&#160;Physical examination revealed severe clinical signs of chronic HF in all animals after 4 - 8 weeks of pacing protocol. Detailed results are summarized&#160;in Table 2.
Initial mean heart rate of sinus rhythm was 100 &#177; 38 beats/min, the mean aortic blood pressure reached 47 &#177; 38 mmHg and CVP 14 &#177; 4 mmHg. Chest X-rays showed heart shadow dilation, with a cardiothoracic ratio of 0.64 &#177; 0.04 (Figure 5A). This is in concordance with transthoracic echocardiography findings. Dilation of all heart chambers, severe systolic dysfunction of both ventricles, and significant mitral and tricuspid regurgitations were apparent on echocardiography. Mean ejection fraction of the left ventricle was below 30% in all animals, the LV wall was judged non-hypertrophic with a thickness of 7 - 10 mm and dyssynchrony of LV contraction was obvious (Figure 6).
Thermodilution measured cardiac output in the resting state was 2.9 &#177; 0.8 L/min and mixed venous blood saturation 62 &#177; 18% corresponded with inadequate tissue oxygen delivery in this model. Average arterial blood flow in the carotid artery was 211 &#177; 144 mL/min and in the subclavian artery was 103 &#177; 108 mL/min. Similarly, regional tissue saturation recorded transcutaneously on the head was only 57 &#177; 13%, and it was even lower on the right forearm, at 37 &#177; 13%.
The pressure volume loop obtained from the PV catheter illustrates the detailed hemodynamic measures and work produced by the mechanical activity of the left ventricle during each cardiac cycle (Figure 4). Maximum LV peak pressure was reduced to 49 &#177; 32 mmHg, but EDP remained low at 7 &#177; 4 mmHg. The measured volumes of the left ventricular chamber were reflective of its dilation and systolic dysfunction. EDV was increased to 189 &#177; 59 mL and ESV to 139 &#177; 37 mL. Averaged SV was 51 &#177; 45 mL and the mean LV ejection fraction was calculated to be 25 &#177; 16%. In addition, a preload independent index of LV contractility can be represented by a dP/dtmax / EDV ratio, which was averaged to 2.2 &#177; 1.7 mmHg/s/mL.
An autopsy confirmed cardiomegaly (Figure 7) with a mean heart weight of 471 &#177; 127 g, which formed 0.7% of body weight. Dilation of all heart chambers and LV wall thinning were stated, and fluid collections were described in pericardial and peritoneal spaces. No shunt or other cardiac anomaly was found in any of the animals.
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/57030/57030fig4.jpg" /> 
Figure 4: Pressure-volume measurements. Samples of direct left ventricular PV loops (A-D) and schematic averaged PV loop of all TIC subjects (E). LV PP = LV peak pressure, EDP = end-diastolic pressure, EDV = end-diastolic volume, and SV = stroke volume. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57030/57030fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/57030/57030fig5.jpg" /> 
Figure 5: Chest X-rays. Enlarged heart shadow (red arrow) and increased cardiothoracic ratio (A). Note the pacing lead introduced to the apex of right ventricle (1), Swan-Ganz catheter placed in the pulmonary artery (2), and PV catheter with 5 electrodes in left ventricular chamber (3). For comparison, a chest X-ray of the normal heart from the day of pacemaker implantation (B). <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57030/57030fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/57030/57030fig6.jpg" /> 
Figure 6: Transthoracic echocardiography. Representative tachycardia-induced cardiomyopathy with severe dilation of all heart chambers (A) and&#160;a similar view obtained before the pacemaker was implanted (B), for comparison. Both acquisitions were taken at end-diastole. Notice the visible tip of pacing lead in RV apex in (A). RV = right ventricle, and LV = left ventricle. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57030/57030fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 7" class="xfigimg" src="/files/ftp_upload/57030/57030fig7.jpg" /> 
Figure 7: Photographs of exposed heart. Cardiomegaly (A) after the TIC induction. Normal porcine heart sample for size comparison (B) (scales in cm). <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57030/57030fig7large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Parameter</td>
			<td colspan="3">TIC value</td>
			<td>Units</td>
		</tr>
		<tr>
			<td>&#160;&#160; Imaging</td>
			<td></td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>CTR</td>
			<td>0.64</td>
			<td>&#177;</td>
			<td>0.04</td>
			<td></td>
		</tr>
		<tr>
			<td>LV EF</td>
			<td></td>
			<td>&#60; 30</td>
			<td></td>
			<td>%</td>
		</tr>
		<tr>
			<td>LV EDD</td>
			<td>66</td>
			<td>&#177;</td>
			<td>3</td>
			<td>mm</td>
		</tr>
		<tr>
			<td>RV EDD</td>
			<td>40</td>
			<td>&#177;</td>
			<td>6</td>
			<td>mm</td>
		</tr>
		<tr>
			<td>AV regurgitations</td>
			<td></td>
			<td>severe</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td colspan="2">&#160;&#160; Circulation parameters</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>HR</td>
			<td>100</td>
			<td>&#177;</td>
			<td>38</td>
			<td>beats/min</td>
		</tr>
		<tr>
			<td>MAP</td>
			<td>47</td>
			<td>&#177;</td>
			<td>38</td>
			<td>mmHg</td>
		</tr>
		<tr>
			<td>CO</td>
			<td>2.9</td>
			<td>&#177;</td>
			<td>0.8</td>
			<td>L/min</td>
		</tr>
		<tr>
			<td>SvO2</td>
			<td>62</td>
			<td>&#177;</td>
			<td>18</td>
			<td>%</td>
		</tr>
		<tr>
			<td>rSO2 head</td>
			<td>57</td>
			<td>&#177;</td>
			<td>13</td>
			<td>%</td>
		</tr>
		<tr>
			<td>rSO2 right forearm</td>
			<td>37</td>
			<td>&#177;</td>
			<td>13</td>
			<td>%</td>
		</tr>
		<tr>
			<td>Carotid flow</td>
			<td>211</td>
			<td>&#177;</td>
			<td>144</td>
			<td>mL/min</td>
		</tr>
		<tr>
			<td>Subclavian flow</td>
			<td>103</td>
			<td>&#177;</td>
			<td>108</td>
			<td>mL/min</td>
		</tr>
		<tr>
			<td>CVP</td>
			<td>14</td>
			<td>&#177;</td>
			<td>4</td>
			<td>mmHg</td>
		</tr>
		<tr>
			<td colspan="2">&#160;&#160; Pressure-volume acquisition</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>LV PP</td>
			<td>49</td>
			<td>&#177;</td>
			<td>32</td>
			<td>mmHg</td>
		</tr>
		<tr>
			<td>LV EDP</td>
			<td>7</td>
			<td>&#177;</td>
			<td>4</td>
			<td>mmHg</td>
		</tr>
		<tr>
			<td>LV EDV</td>
			<td>189</td>
			<td>&#177;</td>
			<td>59</td>
			<td>mL</td>
		</tr>
		<tr>
			<td>LV ESV</td>
			<td>139</td>
			<td>&#177;</td>
			<td>37</td>
			<td>mL</td>
		</tr>
		<tr>
			<td>SV</td>
			<td>51</td>
			<td>&#177;</td>
			<td>45</td>
			<td>mL</td>
		</tr>
		<tr>
			<td>LV EF</td>
			<td>25</td>
			<td>&#177;</td>
			<td>16</td>
			<td>%</td>
		</tr>
		<tr>
			<td>dP/dtmax / EDV ratio</td>
			<td>2.2</td>
			<td>&#177;</td>
			<td>1.7</td>
			<td>mmHg/s/mL</td>
		</tr>
		<tr>
			<td>&#160;&#160; Autopsy</td>
			<td></td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>mean heart weight</td>
			<td>471</td>
			<td>&#177;</td>
			<td>127</td>
			<td>g</td>
		</tr>
		<tr>
			<td colspan="5">cardiomegaly, dilation of heart chambers, LV wall thinning, pericardial fluid collections</td>
		</tr>
	</tbody>
</table>
Table 2: Numerical results of the TIC model after cessation of pacing protocol. All values expressed as mean &#177; standard deviation. CTR = cardiothoracic ratio, LV EF = LV ejection fraction, LV EDD / RV EDD = LV / RV end-diastolic diameter, AV regurgitations = atrioventricular valve regurgitations, HR = heart rate, MAP = mean aortic pressure, CO = cardiac output, SvO2 = mixed venous hemoglobin saturation, rSO2 = regional tissue saturation, CVP = central venous pressure, LV PP = LV peak pressure, LV EDP / LV EDV = LV end-diastolic pressure/volume, LV ESV = LV end-systolic volume, and SV = stroke volume.

Watch this Scientific Journal Video about Tachycardia-Induced Cardiomyopathy As a Chronic Heart Failure Model in Swine at JoVE.com

Tachycardia-Induced Cardiomyopathy As a Chronic Heart Failure Model in Swine

Here, we present a protocol to produce tachycardia-induced cardiomyopathy in swine. This model represents a potent way to study the hemodynamics of progressive chronic heart failure and the effects of applied treatment.

A stable and reliable model of chronic heart failure is required for many experiments to understand hemodynamics or to test effects of new treatment ...

tachycardia-induced-cardiomyopathy-as-chronic-heart-failure-model

Nanyang Technological University

Research

JoVE Journal

Medicine

13.5K Views.  Charles University. Hier presenteren we een protocol voor de productie van tachycardie-geïnduceerde cardiomyopathie in varkens. Dit model vertegenwoordigt een krachtige manier om de hemodynamica van progressieve chronische hartfalen en de effecten van toegepaste behandeling te studeren.

Video: Tachycardia-Induced Cardiomyopathy As a Chronic Heart Failure Model in Swine

Myocardial Infarction and Functional Outcome Assessment in Pigs

Introduction of newly discovered cardiovascular therapeutics into first-in-man trials depends on a strictly regulated ethical and legal roadmap. One important prerequisite is a good understanding of all safety and efficacy aspects obtained in a large animal model that validly reflect the human scenario of myocardial infarction (MI). Pigs are widely used in this regard since their cardiac size, hemodynamics, and coronary anatomy are close to that of humans. Here, we present an effective protocol for using the porcine MI model using a closed-chest coronary balloon occlusion of the left anterior descending artery (LAD), followed by reperfusion. This approach is based on 90 min of myocardial ischemia, inducing large left ventricle infarction of the anterior, septal and inferoseptal walls. Furthermore, we present protocols for various measures of outcome that provide a wide range of information on the heart, such as cardiac systolic and diastolic function, hemodynamics, coronary flow velocity, microvascular resistance, and infarct size. This protocol can be easily tailored to meet study specific requirements for the validation of novel cardioregenerative biologics at different stages (i.e. directly after the acute ischemic insult, in the subacute setting or even in the chronic MI once scar formation has been completed). This model therefore provides a useful translational tool to study MI, subsequent adverse remodeling, and the potential of novel cardioregenerative agents.

This protocol describes the porcine myocardial infarction (MI) model using a 90 min closed-chest coronary balloon occlusion of the left anterior descending artery (LAD), followed by reperfusion. Furthermore, the protocol for several outcome parameters, such as cardiac function, hemodynamics, microvascular resistance, and infarct size, are also presented.

Introduction of newly discovered cardiovascular therapeutics into first-in-man trials depends on a strictly regulated ethical and legal roadmap. One ...

A Model of Cardiac Remodeling Through Constriction of the Abdominal Aorta in Rats

Heart failure is one of the leading causes of death worldwide. It is a complex clinical syndromethat includes fatigue, dyspnea, exercise intolerance, and fluid retention. Changes in myocardial structure, electrical conduction, and energy metabolism develop with heart failure, leading to contractile dysfunction, increased risk of arrhythmias, and sudden death. Hypertensive heart disease is one of the key contributing factors of cardiac remodeling associated with heart failure. The most commonly-used animal model mimicking hypertensive heart disease is created via surgical interventions, such as by narrowing the aorta. Abdominal aortic constriction is a useful experimental technique to induce a pressure overload, which leads to heart failure. The surgery can be easily performed, without the need for chest opening or mechanical ventilation. Abdominal aortic constriction-induced cardiac pathology progresses gradually, making this model relevant to clinical hypertensive heart failure. Cardiac injury and remodeling can be observed 10 weeks after the surgery. The method described here provides a simple and effective approach to produce a hypertensive heart disease animal model that is suitable for studying disease mechanisms and for testing novel therapeutics.

A rat model of abdominal aortic constriction that induces cardiac hypertrophy and remodeling is described. An efficient, highly-reproducible, and minimally-invasive method is used to provide a simple yet useful platform for research in myocardial hypertrophy and dysfunction.

Heart failure is one of the leading causes of death worldwide. It is a complex clinical syndromethat includes fatigue, dyspnea, exercise intolerance, and ...

A Chronic Cardiac Ischemia Model in Swine Using an Ameroid Constrictor

Cardiovascular disease remains the number one cause of mortality in the United States. There are numerous approaches to treating these diseases, but regardless of the approach, an in vivo model is needed to test each treatment. The pig is one of the most used large animal models for cardiovascular disease. Its heart is very similar in anatomy and function to that of a human. The ameroid placement technique creates an ischemic area of the heart, which has many useful applications in studying myocardial infarction. This model has been used for surgical research, pharmaceutical studies, imaging techniques, and cell therapies.
There are several ways of inducing an ischemic area in the heart. Each has its advantages and disadvantages, but the placement of an ameroid constrictor remains the most widely used technique. The main advantages to using the ameroid are its prevalence in existing research, its availability in various sizes to accommodate the anatomy and size of the vessel to be constricted, the surgery is a relatively simple procedure, and the post-operative monitoring is minimal, since there are no external devices to maintain. This paper provides a detailed overview of the proper technique for the placement of the ameroid constrictor.

The purpose of this protocol is to demonstrate the placement of a delayed constricting device (an ameroid constrictor) around a coronary artery in a swine model. This device creates an ischemic area of the heart that is useful for studying new diagnostic imaging techniques and new methods of treatment.

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Surgical Swine Model of Chronic Cardiac Ischemia Treated by Off-Pump Coronary Artery Bypass Graft Surgery

Chronic cardiac ischemia that impairs cardiac function, but does not result in infarct, is termed hibernating myocardium (HM). A large clinical subset of coronary artery disease (CAD) patients have HM, which in addition to causing impaired function, puts them at higher risk for arrhythmia and future cardiac events. The standard treatment for this condition is revascularization, but this has been shown to be an imperfect therapy. The majority of pre-clinical cardiac research focuses on infarct models of cardiac ischemia, leaving this subset of chronic ischemia patients largely underserved. To address this gap in research, we have developed a well-characterized and highly reproducible model of hibernating myocardium in swine, as swine are ideal translational models for human heart disease. In addition to creating this unique disease model, we have optimized a clinically relevant treatment model of coronary artery bypass surgery in swine. This allows us to accurately study the effects of bypass surgery on heart disease, as well as investigate additional or alternate therapies. This model surgically induces single vessel stenosis by implanting a constrictor on the left anterior descending (LAD) artery in a young pig. As the pig grows, the constrictor creates a gradual stenosis, resulting in chronic ischemia with impaired regional function, but preserving tissue viability. Following the establishment of the hibernating myocardium phenotype, we perform off-pump coronary artery bypass graft surgery to revascularize the ischemic region, mimicking the gold-standard treatment for patients in the clinic.

This protocol presents a surgical large animal model of chronic, single vessel ischemia that results in regional abnormalities but does not create infarct, known as hibernating myocardium. Following establishment of chronic ischemia, animals are treated with off-pump LIMA-LAD coronary artery bypass graft surgery to revascularize the ischemic tissue.

Chronic cardiac ischemia that impairs cardiac function, but does not result in infarct, is termed hibernating myocardium (HM). A large clinical subset of ...

Establishing a Swine Model of Post-myocardial Infarction Heart Failure for Stem Cell Treatment

Although advances have been achieved in the treatment of heart failure (HF) following myocardial infarction (MI), HF following MI remains one of the major causes of mortality and morbidity around the world. Cell-based therapies for cardiac repair and improvement of left ventricular function after MI have attracted considerable attention. Accordingly, the safety and efficacy of these cell transplantations should be tested in a preclinical large animal model of HF prior to clinical use. Pigs are widely used for cardiovascular disease research due to their similarity to humans in terms of heart size and coronary anatomy. Therefore, we sought to present an effective protocol for the establishment of a porcine chronic HF model using closed-chest coronary balloon occlusion of the left circumflex artery (LCX), followed by rapid ventricular pacing induced with pacemaker implantation. Eight weeks later, the stem cells were administered by intramyocardial injection in the peri-infarct area. Then the infarct size, cell survival, and left ventricular function (including echocardiography, hemodynamic parameters, and electrophysiology) were evaluated. This study helps establish a stable preclinical large animal HF model for stem cell treatment.

We sought to establish a swine model of heart failure induced by left circumflex artery blockage and rapid pacing to test the effect and safety of intramyocardial administration of stem cells for cell-based therapies.

Although advances have been achieved in the treatment of heart failure (HF) following myocardial infarction (MI), HF following MI remains one of the major ...

Post-Myocardial Infarction Heart Failure in Closed-chest Coronary Occlusion/Reperfusion Model in G&#246;ttingen Minipigs and Landrace Pigs

The development of heart failure is the most powerful predictor of long-term mortality in patients surviving acute myocardial infarction (MI). There is an unmet clinical need for prevention and therapy of post-myocardial infarction heart failure (post-MI HF). Clinically relevant pig models of post-MI HF are prerequisites for final proof-of-concept studies before entering into clinical trials in drug and medical device development.
Here we aimed to characterize a closed-chest porcine model of post-MI HF in adult G&#246;ttingen minipigs with long-term follow-up including serial cardiac magnetic resonance imaging (CMRI) and to compare it with the commonly used Landrace pig model.
MI was induced by intraluminal balloon occlusion of the left anterior descending coronary artery for 120 min in G&#246;ttingen minipigs and for 90 min in Landrace pigs, followed by reperfusion. CMRI was performed to assess cardiac morphology and function at baseline in both breeds and at 3 and 6 months in G&#246;ttingen minipigs and at 2 months in Landrace pigs, respectively.
Scar sizes were comparable in the two breeds, but MI resulted in a significant decrease of left ventricular ejection fraction (LVEF) only in G&#246;ttingen minipigs, while Landrace pigs did not show a reduction of LVEF. Right ventricular (RV) ejection fraction increased in both breeds despite the negligible RV scar sizes. In contrast to the significant increase of left ventricular end-diastolic (LVED) mass in Landrace pigs at 2 months, G&#246;ttingen minipigs showed a slight increase in LVED mass only at 6 months.
In summary, this is the first characterization of post-MI HF in G&#246;ttingen minipigs in comparison to Landrace pigs, showing that the G&#246;ttingen minipig model reflects post-MI HF parameters comparable to the human pathology. We conclude that the G&#246;ttingen minipig model is superior to the Landrace pig model to study the development of post-MI HF.

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Sterile Pericarditis in Aachener Minipigs As a Model for Atrial Myopathy and Atrial Fibrillation

Atrial fibrillation (AF) is the most common arrhythmia caused by structural remodeling of the atria, also called atrial myopathy. Current therapies only target the electrical abnormalities and not the underlying atrial myopathy. For the development of novel therapies, a reproducible large animal model of atrial myopathy is necessary. This paper presents a model of sterile pericarditis-induced atrial myopathy in Aachener minipigs. Sterile pericarditis was induced by spraying sterile talcum and leaving a layer of sterile gauze over the atrial epicardial surface. This led to inflammation and fibrosis, two crucial components of the pathophysiology of atrial myopathy, making the atria susceptible to the induction of AF. Two pacemaker electrodes were positioned epicardially on each atrium and connected to two pacemakers from different manufacturers. This strategy allowed for repeated non-invasive atrial programmed stimulation to determine the inducibility of AF at specified time points after surgery. Different protocols to test AF inducibility were used. The advantages of this model are its clinical relevance, with AF inducibility and the rapid induction of inflammation and fibrosis-both present in atrial myopathy-and its reproducibility. The model will be useful in the development of novel therapies targeting atrial myopathy and AF.

We describe a sterile pericarditis model in minipigs to study atrial myopathy and atrial fibrillation (AF). We present surgical and anesthetic techniques, strategies for vascular access, and a protocol to study the inducibility of AF.

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A Surgical Model of Heart Failure with Preserved Ejection Fraction in Tibetan Minipigs

More than half of heart failure (HF) cases are classified as heart failure with preserved ejection fraction (HFpEF) worldwide. Large animal models are limited for investigating the fundamental mechanisms of HFpEF and identifying potential therapeutic targets. This work provides a detailed description of the surgical procedure of descending aortic constriction (DAC) in Tibetan minipigs to establish a large animal model of HFpEF. This model used a precisely controlled constriction of the descending aorta to induce chronic pressure overload in the left ventricle. Echocardiography was used to evaluate the morphological and functional changes in the heart. After 12 weeks of DAC stress, the ventricular septum was hypertrophic, but the thickness of the posterior wall was significantly reduced, accompanied by dilation of the left ventricle. However, the LV ejection fraction of the model hearts was maintained at &gt;50% during the 12-week period. Furthermore, the DAC model displayed cardiac damage, including fibrosis, inflammation, and cardiomyocyte hypertrophy. Heart failure marker levels were significantly elevated in the DAC group. This DAC-induced HFpEF in minipigs is a powerful tool for investigating molecular mechanisms of this disease and for preclinical testing.

The present protocol describes a step-by-step procedure to establish a minipig model of heart failure with preserved ejection fraction using descending aortic constriction. The methods for evaluating cardiac morphology, histology, and function of this disease model are also presented.

More than half of heart failure (HF) cases are classified as heart failure with preserved ejection fraction (HFpEF) worldwide. Large animal models are ...

Translational Rabbit Model of Chronic Cardiac Pacing

Animal models of cardiac pacing are beneficial for testing novel devices, studying the pathophysiology of artificially paced heart rhythms, and studying arrhythmia-induced cardiomyopathies and subsequent heart failure. Currently, only a few such models are available, and they mostly require extensive resources. We report a new experimental cardiac pacing model in small mammals with the potential to study arrhythmia-induced heart failure.
In six New Zealand white rabbits (mean weight: 3.5 kg) under general inhalational anesthesia the jugular region was dissected and a single pacing lead was inserted via the right external jugular vein. Using fluoroscopic guidance, the lead was further advanced to the right ventricular apex, where it was stabilized using passive fixation. A cardiac pacemaker was then connected and buried in a subcutaneous pocket.
The pacemaker implantation was successful with good healing; the rabbit anatomy is favorable for the lead placement. During 6 months of follow-up with intermittent pacing, the mean sensed myocardial potential was 6.3 mV (min: 2.8 mV, max: 12 mV), and the mean lead impedance measured was 744 &#937; (min: 370 &#937;, max: 1014 &#937;). The pacing threshold was initially 0.8 V &#177; 0.2 V and stayed stable during the follow-up.
This present study is the first to present successful transvenous cardiac pacing in a small-mammal model. Despite the size and tissue fragility, human-size instrumentation with adjustments can safely be used for chronic cardiac pacing, and thus, this innovative model is suitable for studying the development of arrhythmia-induced cardiomyopathy and consequent heart failure pathophysiology.

We present a minimally invasive leporine model of long-term cardiac pacing that can be utilized for artificial pacing and heart failure development in preclinical studies.

Animal models of cardiac pacing are beneficial for testing novel devices, studying the pathophysiology of artificially paced heart rhythms, and studying ...

Ascending Aortic Banding for Studying Pressure-Overload Induced Heart Failure

A Minimally Invasive Model of Aortic Stenosis in Swine

Large animal models of heart failure play an essential role in the development of new therapeutic interventions due to their size and physiological similarities to humans. Efforts have been dedicated to creating a model of pressure-overload induced heart failure, and ascending aortic banding while still supra-coronary and not a perfect mimic of aortic stenosis in humans, closely resembling the human condition.
The purpose of this study is to demonstrate a minimally invasive approach to induce left ventricular pressure overload by placing an aortic band, precisely calibrated with percutaneously introduced high-fidelity pressure sensors. This method represents a refinement of the surgical procedure (3Rs), resulting in homogenous trans-stenotic gradients and reduced intragroup variability. Additionally, it enables swift and uneventful animal recovery, leading to minimal mortality rates. Throughout the study, animals were followed for up to 2 months after surgery, employing transthoracic echocardiography and pressure-volume loop analysis. However, longer follow-up periods can be achieved if desired. This large animal model proves valuable for testing new drugs, particularly those targeting hypertrophy and the structural and functional alterations associated with left ventricular pressure overload.

Author Spotlight: Development of a Minimally Invasive Large-Animal Model for Reliable and Reproducible Cardiovascular Research 

This protocol describes a minimally invasive surgical procedure for ascending aortic banding in swine.

Large animal models of heart failure play an essential role in the development of new therapeutic interventions due to their size and physiological ...

Tachycardia-Induced Cardiomyopathy As a Chronic Heart Failure Model in Swine

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