Using Computer-based Image Analysis to Improve Quantification of Lung Metastasis in the 4T1 Breast Cancer Model

Podsumowanie

We describe a more consistent and expeditious method to quantify lung metastasis in the 4T1 breast cancer model by using Fiji-ImageJ.

Streszczenie

Breast cancer is a devastating malignancy, accounting for 40,000 female deaths and 30% of new female cancer diagnoses in the United States in 2019 alone. The leading cause of breast cancer related deaths is the metastatic burden. Therefore, preclinical models for breast cancer need to analyze metastatic burden to be clinically relevant. The 4T1 breast cancer model provides a spontaneously-metastasizing, quantifiable mouse model for stage IV human breast cancer. However, most 4T1 protocols quantify the metastatic burden by manually counting stained colonies on tissue culture plates. While this is sufficient for tissues with lower metastatic burden, human error in manual counting causes inconsistent and variable results when plates are confluent and difficult to count. This method offers a computer-based solution to human counting error. Here, we evaluate the protocol using the lung, a highly metastatic tissue in the 4T1 model. Images of methylene blue-stained plates are acquired and uploaded for analysis in Fiji-ImageJ. Fiji-ImageJ then determines the percentage of the selected area of the image that is blue, representing the percentage of the plate with metastatic burden. This computer-based approach offers more consistent and expeditious results than manual counting or histopathological evaluation for highly metastatic tissues. The consistency of Fiji-ImageJ results depends on the quality of the image. Slight variations in results between images can occur, thus it is recommended that multiple images are taken and results averaged. Despite its minimal limitations, this method is an improvement to quantifying metastatic burden in the lung by offering consistent and rapid results.

Wprowadzenie

One in eight women will be diagnosed with breast cancer in her lifetime, and yet despite multiple treatment options breast cancer is the second leading cause of cancer-related deaths in American women¹. These women are not dying from the primary tumor in their breast. Instead, the metastatic burden is responsible for the mortality of this disease as it commonly spreads to the lung, bone, brain, liver, and lymph nodes². Because of this, breast cancer models need to evaluate metastasis to contribute to curbing the mortality of this disease. The 4T1 murine breast cancer model is a superb protocol to accomplish this. The method described here offers an improvement to the 4T1 model by using Fiji-ImageJ to quantify lung metastasis, producing consistent and expeditious results.

The 4T1 model is well-established, with most labs using protocols such as those described by Pulaski and Ostrand-Rosenberg in 2001³. The 4T1 cell line is 6-Thioguanine (6TG) resistant and representative of stage IV, triple negative breast cancer^3,4,5. It is clinically relevant as it is an orthotopic model and spontaneously metastasizes to the same organs as in human breast cancer^3,4. The 4T1 cells spontaneously metastasize at a predictable rate based on the quantity of cells injected^3,4. Importantly, genetic differences between mice used here caused expected inter-individual variability in metastatic burden. To evaluate metastasis, tissues are harvested to collect and quantify cancer cells in distant sites using 6TG selection and methylene blue staining. The result is a collection of tissue culture plates with blue dots representing metastatic colonies. However, the Pulaski and Ostrand-Rosenberg protocol quantifies metastatic colonies by manually counting them, and therefore this has been the standard means of evaluating metastasis in this model. While this is easy for tissues with low metastatic burden, tissues like the lungs are often laden with metastases. As lung plates can be highly confluent, accurately and precisely quantifying metastatic colonies by manual counting is difficult and prone to human error. To better quantify metastatic burden, we describe using Fiji-ImageJ for a computer-based solution to human counting error. Histopathological analysis with hematoxylin and eosin (H&E) staining is another means to quantify lung metastases, and interestingly has also been improved with Fiji-ImageJ software^6,7. However, because histopathological analysis observes a single slice of the lung, it can be inaccurate and unrepresentative. This is because the 4T1 model causes several metastatic lesions throughout the organ that are not evenly distributed. While overall trends between histopathological analysis and manual counting can be similar⁸, individual values can differ and therefore histopathological analysis should not be used as the sole means of quantification. We demonstrate the benefit compared to histopathological analysis and the inconsistencies in manual counting between different counters, while also demonstrating the consistency of using Fiji-ImageJ. Additionally, we show that this method can reduce the incubation time from 10-14 days to 5 days, meaning researchers can analyze data from their study much sooner than when relying on manual counting.

This method is a collection of simple adjustments to the Pulaski and Ostrand-Rosenberg protocol³. Because the 4T1 model is widely used, and because lung metastasis is a critical parameter to measure in preclinical models, we believe this method can be widely used and is highly valuable to breast cancer researchers. The only additional supplies needed are a camera and access to a computer with Fiji-ImageJ, a free software used frequently in image analysis⁹. This method specifically focuses on lung metastasis, but it could be used for other tissues with significant metastatic burden.

Protokół

All methods described here have been approved by the Institutional Animal Care and Use Committee (IACUC) of Virginia Tech and in accordance with the National Institutes of Health Guide for the Care and Use of Laboratory Animals. Performing this protocol requires permission from the appropriate institutions and adherence to all appropriate guidelines.

1. Cell Culture

1. Make complete culture media (RPMI + 10% Fetal Bovine Serum +1% Pen Strep). Revive 4T1 cells according to ATCC Protocol¹⁰ and incubate at 37 °C and 5% CO₂ in a T-25 flask until confluent. Change media the day after reviving to remove dead cells, and again if media is spent before cells are confluent enough to passage.
2. Once the T-25 flask is confluent, passage cells to a T-75 flask by discarding media, washing flask with 5 mL of 1x Dulbecco’s Phosphate Buffered Saline (DPBS), and adding 500 μL of Trypsin-EDTA. Incubate for 5-10 minutes at 37 °C until cells detach.
   1. Once detached, add 5 mL of warmed complete culture media to cells. Aspirate and transfer the 5 mL to a T-75 flask containing 15 mL of warmed complete culture media.
3. Passage cells in T-75 flasks at least four times. Do this once the flask is confluent by washing with 8 mL of 1x DPBS, adding 1 mL of Trypsin-EDTA for detaching cells, adding 10 mL of warmed media to cells, and diluting 1:6-1:8 into a new T-75 flask containing 20 mL of warmed complete culture media.
4. Passage cells up to the appropriate number of T-150 flasks containing 40 mL of warmed complete culture media for the number of mice to be injected. Most studies will require multiple T-150 flasks to ensure enough cells for injection.
5. When mice are ready to be injected (8 weeks old or weighing over 20 g, depending on the IACUC or institutional protocols), harvest cells by discarding media, washing each flask with 10 mL of 1x DPBS and adding 2 mL of trypsin-EDTA. Incubate for 5-10 minutes at 37 °C until cells detach.
6. Wash flask with 10 mL of complete media and transfer all contents (10 mL of media + 2 mL of trypsin-EDTA cell mixture) to the next flask. Continue to wash and collect cells from each flask using the same 10 mL of media to avoid using an excessive amount of media.
   1. Once all flasks have been collected, transfer the contents into a 50 mL centrifuge tube. Collect a 10 μL sample for counting in a microcentrifuge tube and centrifuge the 50 mL conical tube at 125 x g for 5 minutes.
7. While cells are being centrifuged, add 10 μL of Trypan blue to 10 μL of cell sample. Count cells using a hemocytometer. Once the total number of cells is determined, calculate the concentration of cells needed to inject mice for 1.2 x 10⁶ cells per mouse (per 100 μL).
8. After centrifugation, decant media and resuspend cell pellet in correct amount of sterile 1x DPBS for 1.2 x 10⁶ cells per 100 μL. Split cell/DPBS mixture into microcentrifuge tubes for easy access with the syringe when aspirating cells for injection. Keep cells on ice and inject soon thereafter as cells will begin to die after being on ice for extended periods of time.

2. Injections

1. Prepare cells for injection by tapping or gently mixing the microcentrifuge tube to resuspend the cells, and then aspirate 600 μL into a 1 mL syringe. Turn the syringe upwards and pull the plunger down to bring cells away from the syringe opening. Tap the syringe to rid it of air bubbles.
2. Attach the needle bevel up and dispense cells back into the microcentrifuge tube until only 500 μL remain in the syringe. Put syringe flat on ice.
   NOTE: 4T1 cells fall out of suspension quickly. Therefore, it is important to mix cells back into suspension by tapping frequently.
3. Anesthetize 8 week old/>20 g female BALB/c mouse using isoflurane or other approved anesthetic agent. Monitor the mouse’s breathing to assess depth of anesthesia.
4. Once the mouse is properly anesthetized as indicated by lack of corneal reflex, place the mouse on its back. Using the thumb, pointer, and middle finger, gently hold down the mouse. Use the pointer and middle fingers to hold down the mouse’s upper body and thumb for its rear left leg. Be gentle but firm.
5. With the bevel of the needle up, inject 100 μL of cells subcutaneously into the mouse’s left abdominal mammary fat pad. Monitor for a good bleb and any leakage, and ensure the mouse wakes up and moves easily after injection.
   1. Change needles between each mouse.
      NOTE: Do not allow needle to enter the peritoneal cavity. This would cause the cancer to spread quickly and not be representative of the model. To ensure a subcutaneous injection, gently pull upwards on the needle when inserted in the left abdominal mammary fat pad. If the needle is easily lifted upwards, it is correctly positioned subcutaneously.

3. Monitoring

1. Monitor mice at least 3 times a week for weight, body condition score, tumor size, tumor condition, respiration, activity level, appearance, and movement. Once the tumor reaches 0.7-0.8 cm in diameter, begin to monitor daily.
   1. Consider euthanasia when tumor size reaches 1.5 cm, or weight loss reaches 20%, or severe clinical decline in body condition score, tumor condition, respiration, activity level, appearance, or movement are observed based on institutional guidelines.
      NOTE: Body condition score is crucial to monitor as body weight may increase as the tumor increases in size, negating body condition loss due to disease burden. Exact monitoring protocols will depend on the approved IACUC or institutional protocols.

4. Necropsy

1. Euthanize mouse using CO₂ following institutional guidelines.
2. Spray mouse with 70% ethanol to disinfect. Make an incision up the ventral midline of the mouse to expose the body cavity.
3. Remove the kidney. Continue cutting up the midline until the diaphragm is visible. Use scissors to puncture the diaphragm to deflate the lungs. Trim the diaphragm to get better access to the cavity.
4. Use blunt scissors to cut up the center of the ribcage. Pin ribcage back to expose the lung and heart.
5. Perfuse the heart with 2 mL of non-sterile 1x DPBS by inserting a needle into the apex of the heart until it pools in the abdominal cavity where the kidney was removed.
6. To remove the heart and lungs, use blunt scissors to cut the esophagus and trachea directly above the heart. Using forceps, begin to pull the heart away from the body and cut away at any connective tissue keeping it attached. The lungs will come out with the heart.
7. Identify the multi-lobed (right) and single-lobed (left) lungs. Keep heart attached for reference, but once lungs are identified, cut the heart away.
8. Label a 12 well plate containing 1x Hank’s Balanced Saline Solution (HBSS) in each well. Each mouse needs 2 wells. Place the multi-lobed (right) lung in the 12 well plate for metastasis evaluation and keep on ice. Keep the neighboring well empty for now.
   NOTE: It is important to use the same lung (multi-lobed) from every mouse to ensure each sample is close in size. The single-lobed lung can then be used for other analysis, like histopathology.
   NOTE: Samples are stable on ice or at 4 °C for a few hours.

5. Processing Tissues

NOTE: All steps in this section should be done using sterile technique.

1. Label 1 15 mL conical tube per mouse and add 2.5 mL of type IV collagenase mixture and 30 units of elastase to each tube. To make type IV collagenase mixture, dissolve 2 mg of type IV collagenase per mL 1x HBSS and sterile filter. This can be stored up to 12 months at -20 °C and thawed when needed.
2. Transfer the lung to the second, clean 1x HBSS well for that sample. Swirl using forceps to remove any remaining blood. Transfer clean lung to empty 3.5 cm tissue culture plate. Mince lung with scissors. Rinse plate with 2.5 mL of 1x HBSS, transfer 1x HBSS and lung pieces into a 15 mL conical tube already containing collagenase/elastase cocktail (5 mL total).
3. Incubate for 75 minutes at 4 °C. Continue mixing samples during this time, so place tubes on a rocker or rotating wheel. During this incubation step, label 50 mL centrifuge tubes and 10 cm tissue culture plates for each mouse. If doing a dilution, label enough 10 cm tissue culture plates for the dilutions.
   NOTE: Label the lid of the tissue culture plates. If labeling the plate itself, the writing will interfere with Fiji-ImageJ analysis.
4. Bring volume of each tube up to 10 mL total with 1x HBSS. Pour contents over a 70 μm cell strainer into a 50 mL conical tube for each sample. Use the plunger of a 1 mL syringe to gently grind the sample through the strainer to allow more cells to filter through.
5. Centrifuge for 5 minutes at 350 x g at room temperature (RT). Discard the supernatant and wash pellet with 10 mL of 1x HBSS. Repeat this step twice.
6. Resuspend pellet in 10 mL of 60 μM 6TG complete culture media, either RPMI or IMDM. Plate samples in 10 cm cell culture plates, using a dilution scheme if desired. Incubate at 37 °C, 5% CO₂ for 5 days.
   NOTE: 1:2, 1:10, and 1:100 are common dilutions that will need to be empirically determined based on study parameters.
   CAUTION: 6TG is toxic. Use caution when handling and follow all Environmental Health and Safety guidelines for disposal.

6. Staining plates

1. Pour culture media off plates into appropriate waste container. Fix cells by adding 5 mL of undiluted methanol per plate and incubate for 5 minutes at RT, making sure to swirl methanol so that it covers the entire plate.
   CAUTION: Methanol is hazardous if ingested, inhaled, or is on skin. Use a fume hood for this step.
2. Pour methanol off plates into appropriate waste container. Rinse plates with 5 mL of distilled water per plate and pour water into appropriate waste container. Add 5 mL of 0.03% methylene blue per plate and incubate for 5 minutes at RT, making sure to swirl methylene blue solution so that it covers the entire plate.
3. Pour methylene blue into appropriate waste container. Rinse plates again with 5 mL of distilled water per plate. Turn plates upside down and blot against a paper towel to remove excess liquid. Place plate on its lid and let air dry overnight at RT.
   NOTE: Metastatic colonies will be blue. Once plates are dried, they can be stored at RT indefinitely.

7. Image analysis

1. Remove labeled lids from plates, taking care to ensure clear identification of samples. Line up all stained lung plates on a clean, light surface to take a picture of all of the plates in one image.
2. Take a picture of the collection of plates in a well-lit area, making sure to minimize reflections as the plates are very reflective. Reflections in the plates will influence image analysis and therefore need to be avoided.
   NOTE: Fiji-ImageJ has an upper limit of 2 gigapixels. Most modern smart phones will have sufficient cameras. Do not use a camera less than 8 megapixels. The camera used in this experiment was a 12.2 megapixel on a Google Pixel 2.
3. Crop the image to include the plates, but exclude the lids or anything else in the background of the image. Upload the cropped image into Fiji-ImageJ.
4. Change the image to black and white using the following commands: Image, Adjust, Color Threshold, Thresholding method: Default, Threshold color: B&W, Threshold space: Lab. Unselect the Dark background box. The image should now be black and white. Black represents the light background, and white represents the blue metastatic colonies.
5. Using the Circle tool on the Fiji-ImageJ toolbar, select the area to be analyzed. Draw one circle to use for all of the plates to ensure each plate is analyzed for the same-sized area. Choose a size that maximizes analyzed area on the plates while minimizing the background noise that appears on the edge of the plates. The size appears in the toolbar as it is drawn, so it is possible to make a perfect circle by monitoring the height and the width as the circle is drawn.
6. Analyze the selected circle to determine what percentage of the area is white, which represents the area of the plate that has blue metastatic colonies. Use the following commands:
   Analyze, Analyze Particles, Size (pixel²): 0-Infinity, Circularity: 0.00-1.00, Show: Nothing, and check the Summarize box. Hit OK.
7. Record the % Area result. This is the percentage of the selected area that is white, and therefore represents the metastatic burden.
   NOTE: It is recommended to either save the results in Fiji-ImageJ or copy/paste the entire results page into a separate document. If % Area results are unexpected or suspicious, it is then possible to see if any of the other measurements were also suspicious or if % Area was recorded incorrectly.
8. Move the circle, without altering its size by grabbing it in its center, to the next plate in the picture. Repeat steps 7.6 and 7.7 for all plates in the picture.
9. Repeat steps 7.1 – 7.8 on at least two more images. Once all plates and images have been analyzed, average the % Area results between different images for each plate to mitigate any inconsistencies between pictures.

Wyniki

This method contains simple adjustments from the Pulaski and Ostrand-Rosenberg 4T1 protocol³ and can be visualized in Figure 1. When 3 separate researchers manually counted metastatic colonies for 12 lung plates (1:10 dilution), the results were very inconsistent between different counters (Figure 2A). All researchers were directed to “count the metastatic colonies that appear as blue dots”, yet the inconsistencies demonstrate...

Dyskusje

As demonstrated, manually counting the metastatic colonies on each lung plate can be an inaccurate and imprecise method to quantify lung metastasis, demonstrating the need for a better means of quantification (Figure 2). Histopathological analysis differed slightly from both manual counting and Fiji-ImageJ analysis (Figure 2B and 4D), likely because the H&E slides are not a representative sample of the entire organ. The protocol harvests an ...

Materiały

Name	Company	Catalog Number	Comments
Anesthesia chamber	See comments	See comments	Use approved materials in your institution's policies
Anesthetic agent	See comments	See comments	Use approved materials in your institution's policies
BALB/c Female Mice	The Jackson Laboratory	000651
Blunt scissors	Roboz	RS-6700
Calculator	Any	Any
Camera	Any	Any	Minimum of 8 megapixels
Centrifuge	Any	Any	Needs to be capable of 125 x g and 300 x g
CO2 euthanasia setup	See comments	See comments	Use approved materials in your institution's policies
Cold room, refrigerator, cold storage	Any	Any
Computer with Fiji-ImageJ	Any	Any	Needs to be capable of running Fiji-ImageJ
Counting Chamber	Fisher Scientific	02-671-10
Curved scissors	Roboz	RS-5859
Distilled water	Any	Any
Elastase	MP Biomedicals	100617
Electronic scale	Any	Any
Fetal Bovine Serum (FBS)	R&D Systems	S11150
Forceps	Roboz	RS-8100
Ice	N/A	N/A
Incubator	See comments	See comments	Needs to be capable of 5% CO2 and 37 °C
Methanol	Fisher Scientific	A412SK-4
Methylene blue	Sigma-Aldrich	03978-250ML
Penicillin Streptomycin	ATCC	30-2300
Pins or needles	Any	Any	For pinning down mice during necropsy
Plastic calipers	VWR	25729-670
RMPI-1640 Medium	ATCC	30-2001
Rocker or rotating wheel	Any	Any
Sharp scissors	Roboz	RS-6702
Sterile disposable filter with PES membrane	ThermoFisher Scientific	568-0010
T-150 Flasks	Fisher Scientific	08-772-48
T-25 Flasks	Fisher Scientific	10-126-10
T-75 Flasks	Fisher Scientific	13-680-65
Tri-cornered plastic beaker	Fisher Scientific	14-955-111F	Used to weigh mice
Trypan blue	VWR	97063-702
Trypsin-EDTA	ATCC	30-2101
Type IV collagenase	Sigma-Aldrich	C5138
3.5 cm tissue culture plates	Nunclon	153066
1 mL syringe	BD	309659
1.7 mL microcentrifuge tubes	VWR	87003-294
10 cm tissue culture plates	Fisher Scientific	08-772-22
12 well plate	Corning	3512
15 mL centrifuge tube	Fisher Scientific	14-959-70C
1X Dulbecco's Phostphate Buffered Saline (DPBS)	Fisher Scientific	SH30028FS
1X Hank’s Balanced Saline Solution (HBSS)	Thermo Scientific	SH3026802
27 g 1/2 in needles	Fisher Scientific	14-826-48
4T1 (ATCC® CRL­2539™)	ATCC	CRL-2539
50 mL centrifuge tube	Fisher Scientific	14-959-49A
6-Thioguanine	Sigma-Aldrich	A4882
70 μM cell strainer	Fisher Scientific	22-363-548
70% ethanol	Sigma Aldrich	E7023	Dilute to 70% with DI water