Technique of Minimally Invasive Transverse Aortic Constriction in Mice for Induction of Left Ventricular Hypertrophy

Summary

The aim of this protocol is to describe step-by-step the technique of minimally invasive transverse aortic constriction (TAC) in mice. By elimination of intubation and ventilation which are mandatory for the commonly used standard procedure, minimally invasive TAC simplifies the operative procedure and reduces the strain put on the animal.

Abstract

Transverse aortic constriction (TAC) in mice is one of the most commonly used surgical techniques for experimental investigation of pressure overload-induced left ventricular hypertrophy (LVH) and its progression to heart failure. In the majority of the reported investigations, this procedure is performed with intubation and ventilation of the animal which renders it demanding and time-consuming and adds to the surgical burden to the animal. The aim of this protocol is to describe a simplified technique of minimally invasive TAC without intubation and ventilation of mice. Critical steps of the technique are emphasized in order to achieve low mortality and high efficiency in inducing LVH.

Male C57BL/6 mice (10-week-old, 25-30 g, n=60) were anesthetized with a single intraperitoneal injection of a mixture of ketamine and xylazine. In a spontaneously breathing animal following a 3-4 mm upper partial sternotomy, a segment of 6/0 silk suture threaded through the eye of a ligation aid was passed under the aortic arch and tied over a blunted 27-gauge needle. Sham-operated animals underwent the same surgical preparation but without aortic constriction. The efficacy of the procedure in inducing LVH is attested by a significant increase in the heart/body weight ratio. This ratio is obtained at days 3, 7, 14 and 28 after surgery (n = 6 - 10 in each group and each time point). Using our technique, LVH is observed in TAC compared to sham animals from day 7 through day 28. Operative and late (over 28 days) mortalities are both very low at 1.7%.

In conclusion, our cost-effective technique of minimally invasive TAC in mice carries very low operative and post-operative mortalities and is highly efficient in inducing LVH. It simplifies the operative procedure and reduces the strain put on the animal. It can be easily performed by following the critical steps described in this protocol.

Introduction

Over the past years, the study of heart failure has been conducted in viable animal models¹. Compared to large animal models of heart failure, small animal models have numerous potential advantages. Beside lower costs of housing and maintenance, small animal models are accessible to more researchers due to the less complex facilities needed².

Mouse heart failure models offer many of the same advantages as the rat models. In addition to reduced housing costs³, mouse models benefit from the availability of relevant transgenic and knockout (KO) strains. The possibility of cell type-specific, inducible KO or transgenic strategies make the mouse an invaluable tool to study the pathogenesis of heart failure and to try to identify novel therapeutic regimens³.

Among the mouse models of heart failure currently used⁴, transverse aortic constriction (TAC) which was first described by Rockman⁵ is the preferred model to generate pressure overload-induced left ventricular hypertrophy (LVH)^1,3. The greatest advantage of this model is the ability to allow stratification of LVH², although left ventricular remodeling in response to TAC is variable among different mouse strains. In particular, C57BL/6 mice develop rapid LV dilation after TAC that may not occur with other strains^4,6,7.

The sudden onset of hypertension achieved with TAC causes an approximately 50% increase in LV mass within 2 weeks, allowing to rapidly examine the activity of pharmacological or molecular interventions aiming at modulating the development of LVH⁴. The acute induction of severe hypertension by TAC does not exactly reproduce the progressive left ventricular hypertrophy and remodeling observed in the clinical setting of aortic stenosis or arterial hypertension. Nevertheless, this model is used by many investigators to identify and modify novel therapeutic targets in heart failure⁴.

Performing TAC in mice requires greater surgical expertise than that required for other techniques used to induce LVH and subsequent heart failure². Most authors perform this procedure by intubating and ventilating the animal^2,8, which makes this procedure more demanding and time-consuming and adds to the surgical burden for the animal. Only few investigators have used minimally invasive TAC in their study with brief reference to the surgical procedure^9,10,11.

The aim of this protocol is to describe step-by-step a simplified and user-friendly technique of minimally invasive transverse aortic constriction in mice, highlighting the critical stages of the procedure. By following these key steps, one can easily perform this technique.

Protocol

Male C57BL/6J mice (10 weeks, 25 - 30g, n=60) are used in this protocol. Animals receive humane care in compliance with the guidelines formulated by the French Ministry of Agriculture and of Higher Education and Research, and all procedures are performed in accordance with the European Community Council Directive of November 24, 1986 (86/609/EEC) and the French laws. The protocol was approved by the "Regional Ethics Committee for Animal Experimentation CREMEAS" (#2016092816207606).

1. Preparation for surgery

1. Maintain the mice for one week after arrival in the animal facility on a 12h/12h light/dark cycle, in standard cages, with food (for details see the Table of Materials) and water available ad libitum.
2. On the day of operation, place the mice in individual cages a few minutes prior to induction of anesthesia, in order to avoid any additional stress to the animal. Sterilize all surgical instruments the day before surgery.
3. Inject intra-peritoneally a single dose of a mixture of ketamine (51.4 mg/kg) and xylazine (3.3 mg/kg) diluted in saline solution (0.9% NaCl).
4. Make sure of the depth of the anesthesia by the absence of the toe-retreat reflex.
5. Shave the neck and chest of the animal with a commercially available razor and disinfect the shaved area with 70% alcohol.
6. Place the animal supine on a clean cork working pad and fix the paws with adhesive tape.

2. Surgery

1. Sterile surgical technique is used throughout the procedures. In a spontaneously breathing animal, perform a longitudinal midline cervical incision over 10 mm with an 11-blade knife from supra-sternal notch to the mid-chest in order to expose the sternum (Figure 1).
2. Retract the thyroid by passing a 4/0 monofilament polypropylene stay suture with a Crile-Wood needle holder and tape it to the working pad.
3. Separate bluntly the pre-tracheal muscles with micro-surgical forceps to uncover the trachea.
4. Slide gently the smooth-tipped curved micro-surgical forceps with the closed jaws over the trachea and behind the sternum.
5. By carefully opening and closing the jaws of the smooth-tipped curved microsurgical forceps carry out a blunt dissection under the pre-tracheal muscles and behind the sternum to move the pleura away.
6. Grasp the right supra-clavicular muscles with the smooth-tipped straight micro-surgical forceps and pull up gently the chest of the animal.
7. Slide the inferior jaw of the bone nipper under the sternum and perform a 3-4 mm upper partial sternotomy (Figure 2). Direct the lower part of the mini-sternotomy slightly toward the left.
8. Pass a 7/0 monofilament polypropylene stay suture from inside to outside through the second intercostal space on each side of the mini-sternotomy using a micro-surgical needle holder. Stay close to costo-sternal angle to avoid injury to intercostal and internal thoracic vessels or pleura.
9. Spread the sternal edges using 7/0 monofilament polypropylene stay sutures on each side and fix them to the working pad with adhesive tape.
10. Gently move aside the pre-tracheal muscles, mediastinal fat and thymus using smooth-tipped curved microsurgical forceps to visualize the aortic arch under low-power magnification (2 - 3X) (Figure 3). Take particular care not to touch or damage the parietal pleura to prevent pneumothorax development.
11. Expose the soft tissue under the aortic arch by tying forceps (Figure 4A) and spread gently its jaws. Prepare a tunnel in the soft tissue under the aortic arch with second tying forceps by gently opening and closing the jaws in the soft tissue.
12. Pass a segment of 6/0 silk ligature threaded through the eye of a ligation aid (Figure 4B) held in the left hand under the aortic arch and retrieve it by tying forceps held in the right hand between the origin of the right innominate and left common carotid arteries (Figure 5).
13. Cut a 27-gauge needle to a length of 5 mm and blunt both ends by pressing them with a Crile needle holder. Place the blunted 27-gauge needle next to the aortic arch (Figure 6) with smooth-tipped straight micro-surgical forceps and tie the suture snugly around the needle and the aorta between the right innominate and left common carotid arteries using the two tying forceps (Figure 7). To tie snugly the suture, perform an initial double knot followed by four additional knots. Make sure that all knots are flat.
14. After ligation, remove quickly but gently the needle to achieve a 0.4 mm diameter narrowing and a reproducible transverse 65-70% aortic constriction.
15. Check for hemostasis of the soft tissue around the aortic arch, of the sternal edges and pre-tracheal muscles. Put resorbable hemostatic gauze wherever oozing of blood is observed.Remove the 7/0 monofilament polypropylene stay sutures used for spreading the sternal edges.
16. Pass a simple 6/0 monofilament polypropylene suture with a micro-surgical needle holder from outside to inside of the left second intercostal space and then from inside to outside of the right second intercostal space. Stay close to costo-sternal angle to avoid injury to intercostal and internal thoracic vessels or pleura.
17. Bring together the sternal edges by tying 6/0 monofilament polypropylene suture with a Crile-Wood needle holder.
18. Close the skin with a 5/0 monofilament polypropylene running suture in one layer with a Crile-Wood needle holder.
19. Perform the sham procedure identical to the constriction operation but without tying a suture around the aorta.

3. Post-operative recovery

1. Monitor the animals very closely. Transfer the mouse to an individual cage and place it in a prone position.
2. Allow the mouse to recover under a warming light until fully awake (less than 1 h after inducing anesthesia).
3. For post-operative analgesia, inject 0.1 mg/kg of buprenorphine intraperitoneally. Repeat subcutaneous injections of 0.1 mg/kg of buprenorphine every 8 h for the first three days as indicated.
4. Place the operated mice in standard cages (maximum 3 mice per cage and minimum 2 mice per cage).

4. Heart harvest

1. On the day of analysis, euthanize the mouse with a solution of ketamine 300 mg/kg and xylazine 20 mg/kg in saline by intraperitoneal injection.
2. First harvest the blood from the inferior vena cava and then through the same line inject 5 mL of solution of 2.6 mM EDTA in saline.
3. Harvest the heart, remove the atria and weight the heart (left and right ventricles without atria).
4. Separate the left from the right ventricle with the septum remaining to the left ventricle part. Weigh both tissue samples and freeze them in liquid nitrogen.

Results

Operative and late survival
The operative survival was very high, 98.3% (59 out of 60) for the entire series (TAC and sham-operated animals). The only operative death was due to a bleeding complication in a mouse planed for sham operation. Post-operative survival during the observation period of 28 days was also excellent, by 98.3% (58 out of 59). The only late post-operative death occurred in a TAC mouse on day (D) 16, possibly of cardiac origin.

Discussion

The aim of this protocol is to present a step-by-step illustration of the surgical technique for minimally invasive transverse aortic constriction in mice. Detailed technical description of transverse aortic constriction in mice has been reported by other authors^2,8. However, these investigators perform surgery following intubation and ventilation of animals. The use of an additional step of intubation-ventilation increases the complexity and duration of the whol...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Surgical microscope	Olympus	SZX2-TR30
Razor	Rowenta	Nomad TN3650FO
Sutures:
Polypropylene 7/0	Ethicon	BV-1X
Polypropylene 6/0	BBraun	C0862061
Silk 6/0 ligature	FST	18020-60
Polypropylene 4/0	Ethicon	8683
Polypropylene 5/0	Ethicon	Z303
Drugs:
Ketamin	Merial	Imalgène 1000, LBM154AD
Xylazine	Bayer	Rompun 2%, KP09PPC
Buprenorphine	Ceva	Vetergesic, 072013
Instruments:
Bone nippers	Fine Surgical Tools	16101-10
Ligation aid	Fine Surgical Tools	18062-12
Tying forceps	Fine Surgical Tools	18026-10
Needle holder Crile-Wood	Fine Surgical Tools	12003-15
Microsurgery forceps	Fine Surgical Tools	11003-12
Microsurgery forceps	Fine Surgical Tools	11002-12
Tissue forceps	Fine Surgical Tools	11021-12
Microsurgery needle holder	Fine Surgical Tools	12076-12
Microsurgery scissors	Fine Surgical Tools	91501-09
Mayo scissors	Fine Surgical Tools	14511-15
11-blade knife	Fine Surgical Tools	10011-00
RNA extraction and qPCR:
TriReagent	Euromedex	TR-118-200
Rneasy Mini kit	Qiagen	74704
Qubit Fluorimetric RNA assay	Fisher Scientific	10034622
RNA 6000 Nano kit	Agilent	5067-1511
High Capacity cDNA kit	Fisher Scientific	10400745
Taqman Master Mix	Fisher Scientific	10157154
Taqman BNP primers	Fisher Scientific	Mm01255770_g1
Taqman ANP primers	Fisher Scientific	Mm01255747_g1
Taqman ACE primers	Fisher Scientific	Mm00802048_m1
Taqman Col1a1 primers	Fisher Scientific	Mm00801666_g1
Taqman TGFb primers	Fisher Scientific	Mm01178820_m1
Taqman Gapdh primers	Fisher Scientific	Mm99999915_g1
ABIPrism  Thermocycler	Applied Biosystems	7000
Software:
GraphPad Prism	GraphPad	Prism 7
Animal food
Complete diet for adult rats/mice	Safe	UB220610R