Subconjunctival Administration of Adeno-associated Virus Vectors in Small Animal Models

Summary

In this manuscript, subconjunctival injection is demonstrated as a valid vector delivery method for ocular tissues in mice using an injection system consisting of an infusion/withdrawal syringe pump and a gastight removable syringe coupled with microinjection needles. This injection system is also adaptable for other intraocular administration routes.

Abstract

Ocular diseases include a wide range of inherited genetic and acquired disorders that are appealing targets for local drug delivery due to their relative ease of accessibility via multiple administration routes. Subconjunctival (SCJ) injections offer advantages over other intraocular administration routes as they are simple, safe, and usually performed in an outpatient setting. SCJ injections in small animals usually require the assistance of an operating microscope due to the size of the eye. Previous work has demonstrated that SCJ injection of specific adeno-associated virus (AAV) serotypes is a valid gene delivery strategy for targeted transduction of the ocular surface, eye muscle, cornea, and optic nerve, providing a potential approach for the treatment of many ocular diseases.

Herein, a detailed protocol is presented for SCJ injections in a mouse model using an injection system consisting of a programmable infusion/withdrawal syringe pump (which allows for consistent and precise injection speed and pressure) and a gastight removable syringe coupled with microinjection needles. The injection system is also adaptable for other intraocular administration routes such as intrastromal, intracameral, intravitreal, and subretinal injections in small animals. Although the delivery of adeno-associated viral vectors for ocular gene therapy studies is described, the protocol herein can also be adapted for a variety of ophthalmic solutions in small animal models. The key practical steps in the administration route, setup for the injection platform, preparation of the injection, and tips from direct experience will be discussed in detail. In addition, common validation techniques for AAV delivery confirmation to the desired tissues will also be briefly discussed.

Introduction

Ocular diseases encompass a broad range of both genetic and acquired disorders. In 2015, an estimated 36 million people were legally blind worldwide, and over 1 billion people suffer from at least some level of visual impairment, highlighting the need to scale up alleviation efforts at all levels¹. The main methods for delivering ocular medications include both topical and local administration, such as eye drops or subconjunctival (SCJ), intracameral, intravitreal, and subretinal injections. Although noninvasive topical therapy is the most common delivery method for ophthalmic drugs and is extensively used for many anterior segment disorders, the presence of corneal anatomical barriers presents a challenge for the bioavailability, biodistribution, and efficacy of topically administrated substances, suggesting that it may not be the best candidate treatment route for many diseases of the inner eye. Local injection into the specific ocular compartment affected by the disease is likely to be a more effective and targeted drug delivery approach². However, adverse effects resulting from repeated injections can complicate administration strategies. Ideally, a therapy should maintain long-term therapeutic efficacy following a single administration. Thus, gene therapy is a promising option for minimizing the number of required injections and providing sustained transgene expression for the treatment of ocular disease^3,4.

Numerous viral and nonviral vectors are available for gene therapy; however, AAV vectors are of high interest due to their excellent safety profile. AAV is a small, single-stranded, non-enveloped DNA virus that was initially discovered as a contaminant of an adenovirus preparation in 1965 by Atchison et al.^5,6 AAV was subsequently engineered as an efficient viral vector for gene delivery in the 1980s and has become the gene therapy vector of choice for many diseases, including ocular disorders, over the last few decades. The most notable of these is the first commercially available gene therapy drug, voretigene neparvovec, which was approved by the United States Food and Drug Administration to treat Leber's Congenital Amaurosis, a rare posterior eye disease. Although voretigene neparvovec has successfully overcome barriers to clinical development, challenges remain for the commercialization of additional ocular gene therapies. For example, voretigene neparvovec is administered to patients who retain viable retinal cells via subretinal injection. Thus, patients with more advanced forms of the disease who lack viable retinal cells are not eligible for treatment, as it would provide no clinical benefit. In addition, known complications associated with the subretinal injection procedure were observed, including eye inflammation, cataracts, retinal tearing, maculopathy, and pain^7,8. Other concerns related to this procedure include the possibility of hemorrhage, retinal detachment, endophthalmitis, and revocation of the ocular immune privileged status through eye tissue destruction^9,10,11,12. Thus, efforts to explore less invasive gene delivery routes such as SCJ injection have become increasingly important^{13,14,15,16,17}.

The conjunctiva is a thin membrane containing 3-5 layers of cells and connecting the anterior eye to the interior eyelid. SCJ injections are used clinically for ophthalmic drug delivery to both the anterior and/or posterior segments of the eye for the treatment of ocular diseases such as age-related macular degeneration, glaucoma, retinitis, and posterior uveitis^18,19. They are relatively simple to perform, employed routinely for ophthalmic drug delivery in an outpatient setting²⁰, somewhat painless, do not compromise ocular immune privilege, and allow administered drugs to spread through a large periorbital region that encompasses the optic nerve. Hence, SCJ injections are an attractive route of administration for AAV gene therapy applications. Natural AAV serotypes administered via SCJ injection in mice have previously been characterized for safety, transduction efficiency, serum immunogenicity, biodistribution, and tissue specificity^13,16,21. These data demonstrated that gene delivery to individual ocular tissues via SCJ administration is a formal possibility.

This paper describes a simple and adaptable protocol for SCJ injection to deliver AAV vectors in a mouse model. To ensure the reproducibility of this approach, an injection system consisting of a stereomicroscope, a programmable infusion/withdrawal syringe pump (which allows consistent and precise injection speed and pressure), and a gastight removable syringe coupled with microinjection needles is described. This system is adaptable for other intraocular administration routes such as intrastromal, intracameral, intravitreal, and subretinal injections in small animals. In addition, a fluorescein dye is often utilized to allow for visualization of the AAV injection site. The key practical steps in the administration route, setup for the injection platform, preparation of the injection, and tips from direct experience will be discussed in detail. Finally, common validation techniques for confirmation of AAV delivery to the desired tissues will be briefly discussed.

Protocol

All animal procedures were performed in accordance with the regulations of the Institutional Animal Care and Use Committee at the University of North Carolina at Chapel Hill. The use of AAV vectors is a Biosafety Level 1 biohazard risk. Wear proper personal protective equipment, including a lab coat, gloves, and goggles when handling AAV. For the experiment described herein, a recombinant AAV vector packaged with the serotype 8 capsid and encoding a generic ubiquitous cytomegalovirus (CMV) promoter controlling the expression of green fluorescence protein (GFP) was utilized.

1. AAV vector handling and storage

1. Store the virus in a -80 °C freezer in 100 µL aliquots in siliconized or low-retention microcentrifuge tubes.
2. Thaw all vector stock solutions on ice before use.
   ​NOTE: Dyes such as sodium fluorescein solution (at a final concentration of 0.1-2%) are often mixed with the AAV vectors to visualize the injected solution. Additionally, visualization of injected solutions helps detect air bubbles and monitor AAV distribution and/or leakage after injection.

2. Subconjunctival (SCJ) injection

1. Assemble the injection system.
   1. To assemble the injection system, place a stereomicroscope and a syringe pump in a biosafety cabinet.
      NOTE: An infusion pump is needed to perform injections with high precision. Herein, a Standard Infuse/Withdraw Programmable Syringe Pump is utilized (see the Table of Materials), which includes a tight grip and a secure syringe clamp for syringes ranging in volume from 0.5 µL to 60 mL. This pump also offers enhanced flow performance with high accuracy and smooth flow rates from 1.28 pl/min to 88.28 ml/min.
   2. Cut the polyethylene tubing to a length of approximately 50 cm (see the Table of Materials).
   3. Insert the hub end of a 36 G needle into one of the ends of the tubing.
      NOTE: Slide the needle hub end into the tube for ~3 mm to ensure that no leakage occurs. The 36 G needle is used for the subsequent SCJ injection. Needles ranging between 32 G and 36 G are the most commonly used sizes for SCJ injections. The use of a hemostat to assist this step is highly recommended to avoid the potential risk of sharps injury.
   4. Fill a disposable 3 mL syringe with sterile water; insert this disposable syringe into the side of the tube opposite the needle and flush the water throughout the tubing/needle. Repeat this step with 70% alcohol.
   5. Repeat step 2.1.4 three more times, alternating flushes with sterile water and 70% alcohol, to disinfect the tubing and ensure no leaks, clogs, or damage are observed throughout the tubing.
   6. Use the disposable 3 mL syringe to fill the tubing with sterile water and leave the tubing attached to the disposable syringe.
   7. Place a piece of parafilm on the bench surface and add a pool of sterile water to it (~1 mL). Submerge the portion of the tubing connected to the needle into the pool of sterile water. Pull the disposable syringe out from the tube opening at the opposite end to prevent any air from entering the tubing/needle system upon removal of the syringe. Leave the portion of the tubing connected to the needle submerged in the pool of water.
      NOTE: Perform procedures 2.1.4 to 2.1.7 in a laminar hood.
   8. Fill a 10 µL Hamilton syringe/needle with sterile water and avoid air in the syringe. Connect the Hamilton syringe/needle to the remaining open end of the tubing by submerging the tubing and needle tip of the Hamilton syringe into the pool of sterile water on the parafilm.
   9. Press the fast reverse button on the pump screen to move the pusher block to the approximate length of the syringe. Unscrew the bracket clamping knobs to loosen the retaining brackets on the pusher and the syringe holder blocks. Load the Hamilton syringe onto the syringe holder block and secure the syringe following the manufacturer's instructions.
      NOTE: To secure the syringe, the syringe barrel clamp should be tight against the syringe barrel; however, do not overtighten, especially when using glass syringes. The syringe plunger should be secured by the pusher block retaining bracket.
   10. Adjust the parameters in the pump settings screen.
       1. Press the Force button, and set the force level at 30%. Accept the changes to go back to the settings screen.
       2. Press the quick start button and select Method | Infuse/withdraw.
       3. For the Syringe, select Hamilton 1700, glass, 10 µL. Select the infusion and withdraw rate and the injection volume.
          NOTE: The Force level is set depending on the syringe type/material/capacity/manufacturers; see factory manufacturer instructions for suggested force for each syringe. The injection speed used in this experiment was 200 nL/s. SCJ injections are relatively safe, and there is less of a concern for the induction of elevated intraocular pressure (IOP) resulting from the injection. A slower injection speed is often desirable for certain applications to avoid reflux into the needle and maintain consistency in injections among animals.
   11. Eject the water from the Hamilton syringe but leave the tubing and injection needle full of water. Slightly pull back on the Hamilton syringe by pressing the Reverse button to introduce a small air bubble in the tubing/needle.
       NOTE: The air bubble will serve as a barrier between the water in the tube and the therapeutic drug (in this case, AAV), ensuring the accuracy of the administered dose.
   12. Withdraw the virus by placing the injection needle into an aliquot of the virus stock. Ensure that a visible air bubble remains between the virus and the water in the tubing.
       NOTE: AAV vectors can bind to the plastic tubing and metal needle, leading to a loss of virus and/or inaccurate dosing regimens. Thus, to ensure rigor, reproducibility, and an accurate dose of AAV, precoating the surfaces that subsequently come into contact with the AAV is recommended. To coat the tubing/needle system with the virus, draw the viral vector solution into the tubing/needle and incubate it at room temperature for 10 min to allow for saturation of virus binding to the wall of the needle and/or tubing. Discard the virus.
2. Virus injection
   1. Anesthetize the mouse with inhaled anesthesia (isoflurane) or intraperitoneal injection of ketamine/xylazine/acepromazine. Confirm the surgical plane of anesthesia by a lack of response to firm toe pinches.
      NOTE: Use female and/or male C57BL/6J or BALB/c mice that are at least 6 weeks old. Ketamine/xylazine/acepromazine doses are as follows: ketamine at 70 mg/kg, xylazine at 7 mg/kg, and acepromazine at 1.5 mg/kg.
   2. Apply topical anesthesia to the eye that will receive the injection.
      NOTE: Use 0.1% proparacaine hydrochloride and/or tetracaine hydrochloride ophthalmic solution (0.5%) for topical anesthesia.
   3. Apply topical ointment to the other eye that will not receive an injection to prevent dryness and injury.
   4. Position the mouse on the microscopic stage and expose the mouse eye under the stereomicroscope.
   5. Place two fingers on the eyelid and slightly pull it away from the mouse's eye to expose the conjunctiva, which is the inner membrane connecting the eyelid to the sclera.
   6. Grab the conjunctiva with forceps.
   7. Release the eyelid and hold the needle with the bevel facing upwards using the dominant hand.
   8. Insert the needle into the conjunctiva. Insert the needle until the bevel is completely covered by the conjunctival membrane. Lay the needle against the globe.
      NOTE: As the conjunctiva is a clear membrane, the needle tip/bevel is easily visible.
   9. Start the injection by pressing the Start button using the footswitch.
      NOTE: The movement of the air and the Hamilton plunger are synchronized; any delay indicates excess air in the injecting system or possibly a loose connection between the tubing, needle, and/or syringe components.
   10. After the injection is finished, hold the needle in place for 10 s before withdrawing the needle from the conjunctiva to decrease the chances of backflow.
       NOTE: It is common for a bleb to appear at the site of the SCJ injection. Such blebs normally resolve completely within a few hours post injection.
   11. Put a drop of the topical lubricant gel on the mouse's eyes to prevent ocular dryness/injury, and then place the mouse on a heating pad to recover.
   12. Perform ocular examinations such as tear production, IOP, and slit-lamp examination in conjunction with corneal fluorescein staining to assess ocular abnormities following the injection.
       NOTE: Tear production is measured by a Phenol Red Thread test, and a tonometer is often used to examine the IOP of the mouse eye. It is reported that some intraocular injections, such as intravitreal injections, might result in a significant increase in IOP; however, IOP changes after SCJ injection are not obvious^13,22,23,24.
3. AAV biodistribution and transduction efficiency examination following subconjunctival injection
   1. To investigate the viral genome biodistribution and/or transduction profile of AAV vectors delivered via SCJ, euthanize the mice by AVMA approved method.
      NOTE: In this experiment, the mice were sacrificed 8 weeks post injection.
   2. For biodistribution and transgene expression in targeted ocular compartments, dissect the relevant tissue of interest such as the eyelids, cornea, conjunctiva, eye muscle, retina, and optic nerve. Flash-freeze all tissues and store at -80 °C. To examine whole-body AAV biodistribution, collect organs such as the submandibular lymph nodes and liver, and flash-freeze and store them at -80 °C.
   3. Using a DNA/RNA extraction kit, collect gDNA and RNA from the same sample to examine transgene expression and AAV biodistribution, respectively. If only vector biodistribution is desired, use a DNA extraction kit to extract gDNA.
   4. Perform standard qPCR and RT-qPCR to determine the AAV vector biodistribution and cDNA abundance using vector transgene-specific primers/probes^13,25.
   5. For histology analysis, fix the eyes, embed them in paraffin, and section them at a thickness of 5 µm. Perform standard immunofluorescence staining to reveal transgene expression²⁶.

Results

Solution injected into the subconjunctival space presents as a bleb depending on the injection volume.
In this experiment, 7 µL of AAV (7 × 10⁹ viral genomes (vg)/eye) mixed with fluorescein at a final concentration of 0.1% was injected with a 36 G needle under a stereomicroscope, and the injection speed/pressure was held constant using a programmable syringe pump at 1 µL/s. A bleb can appear upon injection (arrow). A microscopic view of AAV vector administration to the murine SCJ compartm...

Discussion

AAV-mediated gene therapy holds great potential for the treatment of ocular diseases. Current ocular gene therapy relies on two major local administration routes, intravitreal and subretinal injections. Unfortunately, both routes are invasive and can cause serious complications, including retinal detachment, cataract formation, and endophthalmitis. Thus, the investigation of relatively less invasive routes, such as SCJ injection, is of great interest.

Although this technique is relatively stra...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
36 G NanoFil Needles	World Precision Instruments	NF36BV-2
AAV vector	University of North Carolina at Chapel Hill	/
Acepromazine	Henry Schein	NDC 11695-0079-8
anti-GFP antibody	AVES labs Inc.
Digital camera	Cannon	Cannon EOS T5i
DNA/RNA extraction kit	Qiagen	80204
Forceps	Fine Science Tools	F6521
Hamilton syringe	Hamilton	7654-01
India ink	StatLab	NC9903975
Ketamine hydrochloride injection solution	Henry Schein	NDC 0409-2051-05
Moisture-resistant film	Parafilm	807-6
Polyethylene tubing	Becton Dickinson and Company	427401
Proparacaine 0.1%	Bausch Health US	NDC 24208-730-06
Rebound tonometer	Tonovet	/
Sodium fluorescein solution	Sigma-Aldich	46960
Standard Infuse/Withdraw Pump 11 Pico Plus Elite Programmable Syringe Pump	Harvard Bioscience	70-4504
Stereo microscopye	Leica	Mz6
Tetracaine Hydrochloride Ophthalmic Solution 0.5%	Bausch and Lomb	Rx only
Topical ointment	GenTeal	NDC 0078-0429-47
Xylazine	Akorn	NDC 59399-110-20
Zone-Quick Phenol Red Thread Box 100 Threads	ZONE-QUICK	PO6448