A Rabbit Aortic Valve Stenosis Model Induced by Direct Balloon Injury

Summary

An appropriate animal model is needed to understand the pathologic mechanisms underlying aortic valve stenosis (AVS) and to evaluate the efficacy of therapeutic interventions. The present protocol describes a new procedure for developing the AVS rabbit model via a direct balloon injury in vivo.

Abstract

Animal models are emerging as an important tool to understand the pathologic mechanisms underlying aortic valve stenosis (AVS) because of the lack of access to reliable sources of diseased human aortic valves. Among the various animal models, AVS rabbit models are one of the most commonly used in large animal studies. However, traditional AVS rabbit models require a long-term period of dietary supplementation and genetic manipulation to induce significant stenosis in the aortic valve, limiting their use in experimental studies. To address these limitations, a new AVS rabbit model is proposed, in which stenosis is induced by a direct balloon injury to the aortic valve. The present protocol describes a successful technique for inducing AVS in New Zealand white (NZW) rabbits, with step-by-step procedures for the preparation, the surgical procedure, and the post-operative care. This simple and reproducible model offers a promising approach for studying the initiation and progression of AVS and provides a valuable tool for investigating the underlying pathological mechanisms of the disease.

Introduction

It is increasingly recognized that the use of appropriate animal models can contribute to a better understanding of the pathological mechanisms underlying aortic valve stenosis (AVS) due to the lack of access to reliable sources of diseased human aortic valves associated with the progression of aortic stenosis (AS). Among the various animal models for studying AVS, rabbits are one of the most commonly used large-animal AVS models, and the AVS rabbit model is induced either through cholesterol/vitamin D2 supplementation or genetic manipulation^1,2,3,4.

Although rabbit AVS models have provided significant insight into the development and progression of AVS, it still remains challenging to induce AVS consistently and reproducibly, as seen in our preliminary experiments.

In addition to diet-induced and genetically susceptible animal models, a new model of AVS has been established through direct mechanical injury in mice^5,6. The mechanical injury model successfully induces aortic stenosis and represents a simple and reproducible AVS model in wild-type mice. To the best of our knowledge, there have been no prior studies examining the effects of a mechanical injury on the aortic valve in rabbit models. Thus, this study provides a new procedure for inducing AVS in male New Zealand white rabbits through a direct balloon injury to the aortic valve, which can accurately mimic the condition of valvular aortic stenosis. This protocol includes step-by-step descriptions of the preparation, the surgical procedure, and the post-operative care, which are useful for inducing reproducible AVS rabbit models.

Protocol

All animal research procedures were approved and performed in accordance with the Laboratory Animals Welfare Act, the Guide for the Care and Use of Laboratory Animals, and the Guidelines and Policies for Animal Experiments provided by the Institutional Animal Care and Use Committee (IACUC) at the College of Medicine of The Catholic University of Korea (approval number: CUMC-2021-0176-05). The present study utilized 3 month old male New Zealand white (NZW) rabbits weighing 3.5-4.0 kg, which were maintained under standard conditions in individual cages. The rabbits were fed either a normal diet or a 0.5% cholesterol-enriched diet supplemented with 50,000 U of vitamin D2 (see Table of Materials). The experimental design and analysis methods for the induction of the AVS rabbit model are depicted in Figure 1.

1. Preparation for the operation

1. Ensure that all the medical and surgical instruments (see Table of Materials) are sterilized at the beginning of the operation.
2. Prepare the dilation balloon catheter set following the steps below.
   1. Connect the in-deflation device filled with a mixture of saline and commercially available contrast medium (1:1) to the luer lock part of the balloon catheter (see Table of Materials).
   2. Fill the balloon with inflation solution, and remove any air from the balloon catheter.
      ​NOTE: For the present study, the inflation solution consisted of 30% iodixanol with 0.9% saline (see Table of Materials).
   3. Verify proper balloon inflation by purging the balloon lumen with the inflation solution.

2. Surgical procedure for the aortic valve injury

1. Administer an intramuscular injection of tiletamine & zolazepam (15 mg/kg) and xylazine (5 mg/kg) (see Table of Materials) to anesthetize the animal.
   NOTE: Before administering the anesthesia, the rabbits were pre-treated with a subcutaneous glycopyrrolate injection (0.05 mg/kg) as a pre-anesthetic anticholinergic agent. The adequate anesthesia level was determined by a combination of criteria, including a lack of response to a toe pinch and a steady respiratory rate.
2. Insert a 24 G intravenous (IV) catheter into the marginal auricular vein, and connect an infusion set with heparinized saline (100 U/kg heparin).
3. Connect the rabbit with a multiparameter veterinary monitor (see Table of Materials) to continuously monitor the vital signs, such as the oxygen saturation signal (SpO₂), temperature, and blood pressure.
   NOTE: For the SpO₂ monitoring, attach the SpO₂ sensor to the rabbit's tongue. For the temperature monitoring, insert the probe into the rabbit's rectum. For the blood pressure monitoring, place the cuff on the forelimb.
4. Place the rabbit in a supine position on an operating table equipped with a C-arm fluoroscopy (see Table of Materials), and remove the hair from the ventral neck area using animal hair clippers (Figure 2A).
5. Sterilize the incision area with iodine, and cover the rabbit with surgical towels.
6. Position the rabbit's heart at the center of the C-arm image.
   NOTE: All researchers must wear protective gear with attached thermoluminescent dosimeters (TLDs) to reduce radiation exposure while performing the C-arm-guided surgery.
   1. Turn on the C-arm, and select the fluoroscopic mode for cardiac imaging.
   2. Adjust the position of the rabbit to ensure that the heart is at the center of the imaging field.
7. Make a longitudinal incision of approximately 3 cm in the skin of the neck, and use surgical scissors to cut the fascia and fat tissue.
8. Expose the left common carotid artery (LCCA) by carefully separating the muscles until approximately 3-3.5 cm of the LCCA is exposed (Figure 2B).
9. Ligate the LCCA with a 3-0 silk suture (see Table of Materials) at the top and end of the exposed LCCA to stop the blood flow.
10. Insert a 22 G IV catheter into the LCCA, and introduce a guide wire (0.016 in, see Table of Materials) into the left ventricle (LV) through the IV catheter, ensuring that the tip of the catheter is properly positioned in the imaging field of the C-arm.
    NOTE: When inserting the IV catheter, carefully loosen the ligature suture on the way down to the aortic valve to allow for the advancement of the catheter.
11. Withdraw the IV catheter, leaving the guide wire, and place a 4-F sheath (see Table of Materials) over the guide wire into the LCCA to introduce the balloon catheter (Figure 2C).
    NOTE: After replacing the IV catheter with the sheath, any trapped air should be removed from the sheath device.
12. Carefully insert the 8 mm balloon catheter over the guidewire into the aortic valve under C-arm fluoroscopic guidance (Figure 2D).
13. Place the balloon catheter tip approximately 1-2 cm distal to the aortic valve, and inflate the balloon by purging the inflation solution with a pressure inflator at 6 atm.
14. Advance the balloon into the LV apex, and pull it back into the LV outlet. Repeat this procedure five times, and then deflate the balloon (Figure 2E, F).
15. Repeat steps 2.8-2.9 three times to ensure adequate valve injury.
16. Withdraw the balloon catheter and guidewire. Slowly remove the sheath from the LCCA, and immediately tie the LCCA with the suture on the way down to the aortic valve.
17. Clean the incision area with saline to remove the blood clots, and inspect the punctured site for arterial bleeding.
18. Close the muscle and skin with a 3-0 non-absorbable suture, and sterilize all the sides of the wound with iodine.

3. Post-operative care

1. Remove the monitoring patches and clips, and keep the rabbit in an intensive care incubator.
   NOTE: After surgery, the rabbits were closely observed for 1 day in an intensive care incubator and then moved to a home cage.
2. Manage post-operative pain with 5 mg/kg tramadol and 3 mg/kg ketoprofen and administer antibiotics (4 mg/kg gentamicin) twice daily for 3 days via subcutaneous injection (see Table of Materials).
   NOTE: Post-operative pain management should adhere to veterinary and IACUC guidelines (e.g., opioid, NSAID, local anesthetic or combination).
3. Feed a 0.5% cholesterol-enriched diet with 50,000 U of vitamin D2 (HC + VitD2) for 8 weeks.

4. Echocardiography

1. After 8 weeks of balloon injury, anesthetize the rabbit using the same procedure described in step 2.1.
2. Visualize the aortic valves using two-dimensional transthoracic views, and record M-mode images in short-axis and long-axis views.
   1. Place the rabbit in a supine position on an echo table.
   2. Shave the chest area using clippers and hair removal cream.
   3. Apply ultrasound transducer gel (see Table of Materials) to the chest.
   4. Adjust the transducer to obtain the parasternal long-axis view and the parasternal short-axis view of the aortic valve.
   5. Use M-mode imaging to record images of the aortic valve in both long-axis and short-axis views, and save the images for later analysis.

5. Histological analysis

1. After the echocardiography, euthanize the rabbit by administering an intravenous injection of potassium chloride (KCl, 3 g/20 mL, 1 mL).
2. Open the thoracic cavity, harvest the heart with the ascending aorta⁷, and place it on ice in phosphate-buffered saline (PBS).
3. Immediately immerse the heart in a 4% paraformaldehyde (PFA) solution, and embed it in a paraffin block (see Table of Materials).
4. Cut the paraffin-embedded heart block into 4 µm thick sections using a microtome, and stain the sections with Masson's trichrome (MT), Alizarin Red, and von Kossa (see Table of Materials) to assess the collagen deposition and valve calcification, respectively^8,9.

Results

Rabbit AVS model induced by aortic valve injury
To induce the rabbit AVS model, male NZW rabbits weighing 3.5-4.0 kg were used for this study. According to the surgical procedures described in step 2 (Figure 2), the AVS model was established by aortic valve injury, which resulted in mechanical aortic valve degeneration and calcification. The control group included rabbits fed with a 0.5% cholesterol-enriched diet (high-cholesterol, HC) and 50,000 U of vitamin D2 (VitD2...

Discussion

Animal AVS models are commonly used to study the pathological aspects of AVS, including the initiation and progression of AVS. This protocol introduces a new rabbit AVS model induced by a direct balloon injury to the aortic valve. In this study, the aortic valve injury model showed significant leaflet thickening and calcification. Compared to the mild AVS model induced by dietary supplementation, the aortic valve in the direct balloon injury model was selectively injured, leading to thickened cusps and restricted motion,...

Materials

Name	Company	Catalog Number	Comments
3-0 Silk suture	AILEE	SK312
4% paraformaldehyde(PFA)	Intron	IBS-BP031-2
Alizarin red Solution	Millpore	TMS-008-C
ASAHI SION BLUE	ASAHI		Guide wire
Back Table Cover	Yuhan kimberly	80101-30
Balloon In-deflation Device	Demax Medical	DID30s
Bionet Veterinary monitor	BIONET	BM3 VET
C-Arm	SIEMENS Healthcare GmbH	Cios alpha
Certified Rabbit Diet	Purina	5322	4.7% Hydrogenated Coconut Oil, 0.5% Cholesterol, & 1% Molasse
Curadle Smart Incubator	Autoelex	CS-CV206	Intensive Care Unit (ICU)
Ergocalciferol	Sigma-aldrich	E5750	Vitamin D2
Fechtner conjunctiva forceps titanium	WORLD PRECISSION Instrument	WP1820
Forceps	HEBU	HB203
Gentamicin	Shin Poong
Glycopyrrolate	SamChunDang
Greenflex NS	DAI HAN PHARM		Normal saline 500 mL
Hematoxylin solution	Sigma-aldrich	HT1079-1 SET
Heparin	JW pharmaceutical		25,000 U
Infusion set for single use	SWOON MEDICAL
Iodine	Green pharmaceutical
Iodixanol	GE Healthcare	Visipaque	Inflation solution (contrast agent)
IV catheter 22 G	BD	382423
IV catheter 24 G	BD	382412
Ketoprofen	SamChunDang
Luer-Lok syringe 10 mL	Becton Dickinson Medical
Luer-Lok syringe 3 mL	Becton Dickinson Medical
Microscope	OLYMPUS	SZ61
Microtome	ThermoFisher Scientific	HM 325
MT stain kit	Sigma-aldrich	HT15-1kt
Needel holder	Solco	009-1304
Needle Holder with Lock and Suture	JEUNGDO BIO & PLANT	H-1222-18
Paraffin	LK LABKOREA	H06-660-107
PBS	Gibco	10010-023
Potassium chloride 40	Daihan Pharm		KCl
Prelude Ideal Hydrophilic Sheath	MERIT MEDICAL	PID4F11018SS	Sheath 4F
PTA Balloon Dilatation catheter	Boston Scientific	H749-3903280208-0	Balloon catheter 8.0 mm
Rompun	Elanco		Xylaxine
sterile Gauze	DAE HAN Medical		10 cm x 20 cm
Surgical Gloves	Ansell	Ansell
Surgical Gown	Yuhan kimberly	90002-02
Surgical Scissors	Nopa, Germany	AC020/16
Surgical Tape	3M micopore	1530-1
Syringe 1 mL	Shin Chang Medical
Syringe 10 mL	Shin Chang Medical
Tissue cassette	Scilav korea	Cas3003
Transducer gel	SUNGHEUNG	SH102
Tridol	Yuhan Corp.		Tramadol HCl
Ultrasound system	Philps	Affiniti 50
Von Kossa stain kit	Abcam	ab105689
Zoletil 50	Virbac korea		Tiletamine & zolazepam