A Mouse Model of Incompletely Resected Soft Tissue Sarcoma for Testing (Neo)adjuvant Therapies

Summary

In this protocol, we describe a mouse model of incomplete surgical resection of soft tissue sarcoma for testing (neo)adjuvant therapies.

Abstract

Surgery is often the first treatment for many solid tumors. However, local relapses frequently occur following primary tumor resection, despite adjuvant or neo-adjuvant therapies. This occurs when surgical margins are insufficiently tumor-free, resulting in residual cancer cells. From a biological and immunological perspective, surgery is not a null event; the wound healing environment is known to induce both pro- and anti-tumorigenic pathways. As a consequence, preclinical models for drug development aimed at preventing local relapse should incorporate surgical resection when testing new (neo)adjuvant therapies, to model the clinical settings in patients treated with surgery.

Here, we describe a mouse model of incomplete surgical resection of WEHI 164 soft tissue sarcoma that allows testing of (neo)adjuvant therapies in the setting of a wound healing response. In this model, 50% or 75% of the tumor is removed, leaving behind some cancer tissue in situ to model gross residual disease after surgery in the clinical setting. This model allows testing therapies in the context of surgery while also considering the wound healing response, which may affect the efficacy of (neo)adjuvant treatments. The incomplete surgical resection results in reproducible regrowth of the tumor in all mice in the absence of adjuvant therapy. Adjuvant treatment with checkpoint blockade results in reduced tumor regrowth. This model is thus appropriate for testing therapies in the context of debulking surgery and its associated wound healing response and can be extended to other types of solid cancer.

Introduction

Surgery remains the main treatment option for many solid tumors¹, including soft tissue sarcoma^2,3. Despite improvements in cancer surgery techniques, and combinations with (neo)adjuvant therapies, there is still a high risk of cancer relapse and metastasis following primary tumor resection^4,5. In soft tissue sarcoma, relapses occur particularly locoregionally, at the site of surgery, resulting in increased morbidity and mortality. In the clinical setting, it can be difficult to obtain wide enough margins (e.g., due to anatomical constraints), resulting in incomplete resection and subsequent tumor recurrence⁶. Surgical stress and the subsequent process of wound healing are known to create an immunosuppressive tumor microenvironment favorable for tumor recurrence^7,8. Therefore, the discovery and development of new therapies for soft tissue sarcoma, particularly immunotherapies, should ideally take the surgical wound healing response into account.

Most preclinical studies for adjuvant therapies are initially carried out using subcutaneous syngeneic or xenotransplant mouse models, without incorporating the surgical stress and wound healing response^9,10. Therefore, we developed a syngeneic subcutaneous mouse soft tissue sarcoma model incorporating incomplete surgical resection. WEHI 164 fibrosarcoma cells are inoculated subcutaneously, and once tumors are established, we remove 50-75% of the tumor bulk (Figure 1A-E). Tumors consistently re-grow from the remaining tumor. This model allows for testing adjuvant therapies while considering the effect of surgical stress and wound healing. Similar surgical models of incomplete resection have been used in a number of studies by several groups and found to be reproducible and effective^11,12,13. Here, we provide a detailed description of this protocol.

Protocol

Animals used in these experiments were obtained from the Animal Resource Centre (Perth, Western Australia). Animals were maintained under standard pathogen-free conditions at the Harry Perkins Institute of Medical Research Bioresources North Facility (Perth, Western Australia). All experiments were carried out following the protocol as approved by the Harry Perkins Institute of Medical Research Animal Ethics Committee. BALB/c mice of 8-12 weeks of age were used in these experiments. The WEHI 164 fibrosarcoma cell line was obtained from CellBank Australia (Westmead, NSW).

1. Inoculation of cells

1. Preparation of cells and animals
   1. Ensure that the cell line is maintained in the recommended media. For example, maintain WEHI 164 cell line in Roswell Park Memorial Institute (RPMI) 1640 medium supplemented with 2 mM L-glutamine, 10% fetal bovine serum, 20 mM HEPES, 0.05 mM 2-mercaptoethanol, 100 U/mL penicillin, and 100 µg/mL streptomycin.
      NOTE: Passage cells at least 3 and up to 5 times after being removed from cryogenic storage. To ensure an optimum cell viability, cells should be split when they are between 70-80% confluent. Tumor cell lines should be tested for mycoplasma, as infection can alter the cell growth and influence the immune response in vivo.
   2. One day before inoculation, shave mice on the lower right flank using clippers.
      NOTE: Female BALB/c mice, aged between 8-12 weeks, of normal weight (16 -22 grams) were used in this experiment.
   3. On the day of inoculation, harvest WEHI 164 cells when 70-80% confluent by trypsinization.
      1. Aspirate the culture medium from the tissue culture flasks and then add sterile phosphate buffered solution (1x PBS), to remove remaining traces of fetal bovine serum (FBS).
      2. Aspirate the PBS from the tissue culture flasks. Add 3 mL of 0.05% trypsin (for a T75 flask) and then swirl the flask so that the whole surface of flask with cells is covered by trypsin.
      3. Incubate the flask at 37 °C, 5% CO₂ incubator for 3 min. Check cells periodically, by tapping on the sides of the flask to see if cells have dislodged.
      4. Remove flasks from cell culture incubator and add 5 mL of media supplemented with FBS to neutralize the trypsin.
         NOTE: Do not leave cells in trypsin longer than necessary, as this can damage cells and lead to low cell viability.
      5. Pipet suspension multiple times to obtain a single cell suspension. Transfer cell suspension to a conical centrifuge tube.
      6. Pellet cells by spinning at 350 x g for 3 min.
   4. Wash the cells three times in 1x PBS.
      1. Resuspend cells in 50 mL of sterile 1x PBS and wash cells by pipetting cell suspension up and down. Pellet cells by spinning at 350 x g for 3 min.
      2. Aspirate the supernatant and resuspend cells in 15 mL of sterile 1x PBS. Wash cells by pipetting cell suspension up and down. Pellet cells by spinning at 350 x g for 3 min.
      3. Aspirate the supernatant and resuspend cells in exactly 10 mL of sterile 1x PBS. Wash cells as in step 1.1.4.2 and transfer a small amount (approximately 100 µL) of cell suspension to an centrifuge tube for counting. Pellet cells by spinning at 350 x g for 3 min.
   5. Determine the cell number using the Trypan blue exclusion method by either using a hemocytometer or an automated cell counter. Resuspend cells in sterile 1x PBS at a concentration of 5 x 10⁶ cells/mL. Keep cell suspension on ice.
      NOTE: The viability of tumor cells should be equal or above 80 % to ensure reproducible tumor growth.
2. Subcutaneous inoculation
   1. Mix the cell suspension thoroughly and fill a syringe with a 26 G needle with 100 µL of cell suspension (5 x 10⁵ cells) in sterile 1x PBS. Repeat mixing of cells before loading the next syringe.
      NOTE: Keep cells on ice throughout the procedure to maintain viability.
   2. Restrain the mouse appropriately, ensuring access to the lower-right flank. Inoculate the mouse subcutaneously on the shaved lower-right flank.
      NOTE: Make sure the inoculation is not in the peritoneum by lifting the needle slightly, which should be visible under the skin. A bubble-like lump should form under the skin following inoculation.
   3. Monitor mice as required by the applicable ethics approval and perform surgical resection when the tumours have grown to a size of about 50 mm².

2. Partial surgical resection of the tumor

NOTE: This protocol requires TWO researchers; one for surgical procedures (SURGEON), and another for mouse monitoring (ASSISTANT).

1. Surgery setup
   1. On day 12 post inoculation, when tumors have reached a size of approximately 50 mm², dose mice with 100 µL (0.1 mg/kg) of buprenorphine s.c. in the scruff of the neck, 30 minutes prior to surgery.
   2. Set up the surgical area with a heat pad covered with bench coat and set up a nose cone for anaesthesia. Sterilize surgical tools prior to use, and between each animal using a heat bead sterilizer, allowing tools to cool before use. Have the following surgical equipment clean and within easy reach: chlorhexidine, swab, gauze, eye gel, two curved forceps, scissors, clip applicator, clip remover, clip refills (Figure 2A, 2B).
   3. Warm the heating chamber to 37 °C and set up another heat pad for recovery (Figure 2C). Place sterilized tools on a sterile surface such as autoclaved pads.
2. Anesthesia
   1. Place the mouse in the induction chamber and anesthetize the mouse with 4% isoflurane (4% in 100% oxygen at a flow rate of 1 L/min) until the breathing rate slows to approximately 60 breaths per minute (1 per second) (this usually takes <1 min).
      NOTE: Do not leave the mouse in the chamber for too long as that may lead to asphyxiation and death. Only have one mouse under anesthesia at a time.
   2. Transfer the mouse onto the heat pad on the surgery table, place the mouse with its nose in the nose cone and maintain the anesthetic state with 3-4% isoflurane in 100% oxygen at a flow rate of 0.5 L/min. Monitor the breathing rate to ensure that the depth of anesthesia is maintained.
      NOTE: The ASSISTANT must monitor the breathing of the mouse throughout the surgery to ensure the correct level of anesthesia is maintained. Lower the anesthetic concentration if breathing becomes too slow or increase the concentration if the depth of anesthesia is too shallow. If the mouse begins gasping, remove mouse from the nose cone, decrease the anesthetic concentration, and wait until breathing normalises before placing on the nose cone again.
   3. Perform a "pinch test" and "corneal reflex test"¹⁴ to ensure that the mouse is fully anesthetized before commencing surgery.
      NOTE: Movement of any part of the mouse is an indication that the mouse is not fully anesthetized. The animal should immediately be given additional anesthetic by increasing the anesthetic concentration.
   4. Cover the mouse's eyes with a small amount of ophthalmic gel to avoid eye dryness.
3. Surgical procedure (SURGEON)
   1. Swab the surgical area 3 times with alcoholic chlorhexidine. Using forceps and a pair of scissors, make a 1 cm straight incision along the dorsal side, 3 mm away from the tumor (Figure 3A, 3B).
      NOTE: Standardizing the incision to 1 cm in every mouse (using a ruler) allows for even assessment of wound healing between mice. Locating the incision 3 mm away from the tumor allows for subsequent intratumoral adjuvant therapy without leakage from the wound.
   2. Using tweezers, pull away the facia and subcutaneous fatty tissue between the tumor and peritoneum. The subcutaneous tumor is normally attached to the skin-side.
   3. Open the wound by gently holding the skin on the tumor bearing side using tweezers, and "invert" the tumor so that it is visible outside (Figure 3C, 3D).
      NOTE: The section of tumor to be debulked should be closest to the opening, to have enough skin to close the wound. Be careful not to cut the skin when removing the tumor.
   4. Using a pair of scissors, cut away the tumor capsule from the half to remove, starting from the base of the tumor closest to the opening.
   5. For 50% debulk surgery, cut across the middle of the tumor. Using curved forceps, scoop up the section of the tumor to be removed (50%); scoop up any remnants from the debulked area.
   6. For 75% debulk, perform a 50% tumor debulk as in part 2.3.5 above. Then cut in half the remaining 50% of tumor and scoop up 25% of the tumor, using curved forceps as described above.
4. Closing the surgical site
   1. Place the remaining tumor back underneath the skin, and using forceps, pull the skin flaps together and line up the skin along the wound.
   2. Hold the skin together 5 mm from the edge of the wound, and use surgical clips to close the wound, starting on the side closest to the forceps. Apply as many clips as needed to ensure no underlying tissue is exposed. Generally, three to four clips are applied with 2 mm gaps between clips.
      NOTE: If any clips is not well applied, remove it using a clip remover and replace with new clips.
5. Recovery of mice (ASSISTANT)
   1. Allow the mice to recover by putting them into the warm (37 °C) heating chamber.
   2. Place the mouse's cage on the heat pad. Monitor the mice in the heating chamber until they have recovered from the anesthetic (awake and walking) and then put the mice back into the cage. Leave the cage on the heat pad for a further 10 minutes, until the mice have become more active.
   3. Give the mice wet and soft food. Monitor the mice 1 hour after surgery for recovery and ensure clips remain in place. Ensure the cage is half on/half off the heat pad to allow animals to self-regulate temperature while unattended.
   4. Dose mice with 0.1 mg/kg buprenorphine (100 µL subcutaneously in the scruff of the neck), 6-8 hours after surgery (at the end of the day). Monitor mice early the following morning, and dose mice again with 0.1 mg/kg buprenorphine (100 µL subcutaneously in the scruff of the neck). Give more wet food as needed.
   5. Monitor mice daily for the next seven days. Clips may be removed after seven days using the clip remover.
6. Adjuvant or neoadjuvant treatment
   1. Treat mice peri-operatively with (neo)adjuvant therapy at any given time, depending on the treatment of interest.
   2. For example, treat mice with one dose of 100 µg of anti-CTLA-4 intraperitoneally (i.p.) on day 15 after inoculation, or with three doses of 200 µg anti-PD-1 i.p. on day 15, 17 and 19 after inoculation.
7. Experimental controls
   1. When using this model to assess the effects of inflammation/wound healing, consider using the following control groups: 1) No-surgery control (treatments can still be administered intratumorally); 2) Sham surgery control: A surgical incision is made in the skin; the tumor is manipulated and exposed, but no tumor tissue is removed; the wound is closed with clips.

Results

Tumor growth to a size of 50 mm² is an ideal size for partial debulk. The incomplete surgical resection of 50 mm² tumors results in 100% (n=5) reproducible regrowth of the tumors in the absence of adjuvant immunotherapy (Figure 4A). We next used the model to test adjuvant immunotherapies using antibodies against checkpoint molecules Cytotoxic T Lymphocyte Associated Protein 4 (CTLA-4) and Programmed Death Receptor 1 (PD-...

Discussion

We provide a protocol for a mouse model of incomplete surgical resection of soft tissue sarcoma to test peri-operative therapies. We also standardized the surgical incision to allow assessment of wound healing between mice following treatment.

Tumor placement is an important part of this protocol. We have opted for a subcutaneous tumor model to allow easy surgical access to the tumor site and administration of local therapies with minimal burden on the mice. It is also important to ensure that...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
26 gauge 0.5 mL insulin syringe	Becton Dickinson, Australia	326769	None
2-Mercaptoethanol	Life Technologies Australia Pty Ltd	21985023	None
Anaestetic gas machine	Darvall Vet, Australia	SKU: 2848	None
Anti-CTLA-4	BioXcell, USA	BE0164	None
Anti-PD-1	BioXcell, USA	BP0273	None
Buprenorphine Hydrochloride Injection, 0.3mg/mL	RB healthcare UK Limited, UK	55175	Prescription order
Chlorhexidine Surgical Scrub 4%	Perigo Australia, Australia	CHL01449F(scrub	None
Fetal Bovine serum	CellSera, Australia	AU-FBS-PG	None
Forceps Fine 10.5 cm	Surgical house, Western Australia	CC74110	None
Forceps Fine 12 cm Serrated	Surgical house, Western Australia	CC74212	None
Forceps Halsted 14 cm	Surgical house, Western Australia	CD01114	None
Heating chamber	Datesand Ltd, UK	Mini-Thermacage	None
HEPES (1M)	Life Technologies Australia Pty Ltd	15630080	None
Isoflurane	Henry Schein Animal Health, Australia	SKU: 29405	Prescription order
Lubricating Eye Ointment	Alcon	n/a	None
Penicillin/streptomycin 1000X	Life Technologies Australia Pty Ltd	15140122	None
Phosphate Buffered Solution 10x	Life Technologies Australia Pty Ltd	70013-032	None
Reflex 7mm Clips	Able scientific, Australia	AS59038	None
Reflex 7mm Wound Clip Applicator	Able scientific, Australia	AS59036	None
Reflex Wound Clip Remover	Able scientific, Australia	AS59037	None
Rodent Qube Anesthesia Breathing Circuit	Darvall Vet, Australia	#7885	None
Roswell Park Memorial Institute (RPMI) 1640 Medium + L-glutamine	Life Technologies Australia Pty Ltd	21870092	None
Scissors Iris STR 11 cm	Surgical house, Western Australia	KF3211	None
Scissors Iris STR 9 cm	Surgical house, Western Australia	JH4209	None
Small Induction Chamber	Darvall Vet, Australia	SKU: 9630	None
TrypLE express 1x	Life Technologies Australia Pty Ltd	12604-021	None
Germinator 500 Glass Bead Sterilizer	Cellpoint Scientific Inc., USA	5-1460-DK