Ovarian cancer metastasis is characterized by numerous diffuse intra-peritoneal lesions, such that accurate visual quantitation of tumor burden is challenging. Herein we describe a method for in situ and ex vivo quantitation of metastatic tumor burden using red fluorescent protein (RFP)-labeled tumor cells and optical imaging.
Epithelial ovarian cancer (EOC) is the leading cause of death from gynecologic malignancy in the United States. Mortality is due to diagnosis of 75% of women with late stage disease, when metastasis is already present. EOC is characterized by diffuse and widely disseminated intra-peritoneal metastasis. Cells shed from the primary tumor anchor in the mesothelium that lines the peritoneal cavity as well as in the omentum, resulting in multi-focal metastasis, often in the presence of peritoneal ascites. Efforts in our laboratory are directed at a more detailed understanding of factors that regulate EOC metastatic success. However, quantifying metastatic tumor burden represents a significant technical challenge due to the large number, small size and broad distribution of lesions throughout the peritoneum. Herein we describe a method for analysis of EOC metastasis using cells labeled with red fluorescent protein (RFP) coupled with in vivo multispectral imaging. Following intra-peritoneal injection of RFP-labelled tumor cells, mice are imaged weekly until time of sacrifice. At this time, the peritoneal cavity is surgically exposed and organs are imaged in situ. Dissected organs are then placed on a labeled transparent template and imaged ex vivo. Removal of tissue auto-fluorescence during image processing using multispectral unmixing enables accurate quantitation of relative tumor burden. This method has utility in a variety of applications including therapeutic studies to evaluate compounds that may inhibit metastasis and thereby improve overall survival.
Epithelial ovarian cancer (EOC) is the most common cause of death from gynecologic malignancy, with an estimated 21,290 new diagnoses in the U.S. in 2015 and an estimated 14,180 deaths1. The vast majority (> 75%) of women are diagnosed with late-stage disease (stage III or IV) characterized by diffuse intra-peritoneal metastasis and poor prognosis. Disease recurrence in the peritoneal cavity following first-line chemotherapy is also common and represents a major cause of mortality2,3. EOC metastasizes by an unique mechanism involving both direct extension from the primary tumor to neighboring peritoneal organs as well as by dissociation or shedding of cells from the primary tumor surface as single cells or multi-cellular aggregates. Cells are shed into the peritoneal cavity, wherein they resist detachment-induced apoptosis4. Buildup of peritoneal ascites is common, as shed tumor cells block peritoneal lymphatic drainage and tumors produce growth factors that alter vascular permeability. A portion of shed tumor cells attach to the surface of peritoneal organs and structures including intestine, liver, omentum and mesentery, whereupon they anchor and proliferate to produce multiple widely disseminated secondary lesions3,5. Hematogenous metastasis is uncommon. Thus, clinical management commonly consists of cytoreductive surgery including "optimal debulking", defined as resection of all visible tumor (no matter how small). Complete cytoreduction is associated with a significant increase in overall survival6,7 and is associated with the challenge of identification and removal of lesions < 0.5 cm.
Small animal models have proven utility in ovarian cancer research in improving our understanding of disease progression as well in identification of prognostic biomarkers and testing of novel chemotherapies or combination therapy approaches. As the primary site of ovarian cancer incidence and metastasis is the peritoneal cavity, orthotopic models of EOC metastasis involve the analysis and characterization of intraperitoneal disease. Although there have been recent improvements in the ability to image tumor cells, even at the single cell level, there still exist significant difficulties in quantifying the metastatic tumor burden of EOC. These challenges arise due to the number, size and anatomic location of metastatic lesions. Furthermore there exists a need to label cancer cells to distinguish them from normal host cells. Previous studies have utilized antibody-based labeling protocols or transfection of tumor cells with luciferase8,9. Direct fluorescent labeling of cancer cells was first reported by Chishima and coworkers in 199710. Fluorescent labels do not require addition of exogenous substrate and provide exquisite tumor cell specificity, providing a more effective means to track cancer metastasis11,12.
Herein we describe an optical imaging method for quantitative analysis of metastatic disease using a syngeneic orthotopic xenograft model comprised of red fluorescent protein (RFP)-tagged murine ID8 ovarian cancer cells13 and immuno-competent C57/Bl6 mice. We demonstrate a novel method of relative tumor burden quantification combining in vivo and ex vivo imaging with removal of tissue auto-fluorescence. This approach has potential utility in studies designed to evaluate the effect of specific genetic, epigenetic or micro-environmental modifications and/or treatment modalities on organ-specific metastasis of ovarian cancer.
Todos in vivo studies were approved by the University of Notre Dame Animal Care and Use Committee and used female C57/BL6J mice.
1. Murine Ovarian Cancer Cell Culture
2. Intra-peritoneal Injection of ID8 Cells and in vivo Imaging
3. Mouse Dissection and Image Acquisition
4. Quantification of Tumor Burden in the Fluorescence Images
5. Data Analysis
The metastatic mechanism of ovarian cancer is characterized by highly diffuse intra-peritoneal metastasis comprised of numerous lesions of varying size, including multiple small (< 2mm) lesions. Thus, use of RFP-labelled tumor cells (Figure 1) and optical imaging provides an alternative method to manual counting and measurement of lesion size. The development of tumor burden over time can be determined by weekly weighing of mice and measurement of abdominal girth to gauge potential presence of ascites. In vivo optical imaging provides a complementary approach to assess tumor burden (Figure 2). Ovarian cancer metastasizes to multiple sites in the peritoneal cavity and molecular drivers of site-specific metastasis are currently unknown. In addition to determination of overall tumor burden, following sacrifice careful dissection can be performed to evaluate and quantify site-specific patterns of metastasis. Thus, optical imaging of peritoneal organs in situ (Figure 3A,B) combined with ex vivo assessment of individual organs (Figure 3C,D) can provide useful data on overall vs organ-specific tumor burden. The scans presented in Figure 3 represent the results of scanning the abdominal cavities and individual organs of mice with varying degree of tumor burden. For example, Figure 3C shows the most tumor burden in the omentum/pancreas, ovaries and mesentery of Mouse A. When compared to those same organs in Mouse B, a significant difference in signal is seen (Figure 3D). The use of the organ scanning template (Figure 4) aids in identification of organ-specific tumor burden. The observation of differential tumor burden is confirmed quantitatively both in terms of tumor surface area and tumor signal intensity (Table 1, Figure 5).
The results shown in these figures and table were analyzed using a minimum and maximum display range of 0 to + 35353 so as to avoid any false-positive signals and auto fluorescence given off by the tissues. The varying degrees of signal seen in Figure 2 and 3 illustrate the large range of tumor burden that can be imaged and quantified using this method. The data in Table 1 illustrates this large range of applicability in quantifying both tumor surface area and signal intensity of the tumor. For example, when looking at the omentum/pancreas of Mouse A compared to that of Mouse B, the normalized tumor surface area is 26 times greater in Mouse A than Mouse B. Furthermore, the large range of signal intensity is also exemplified in the omentum/pancreas of Mice A and B; the normalized raw integrated density of Mouse A is 56 times greater than that of Mouse B. These results demonstrate the validity of comparing the tumor burden of several test subjects relative to each other, in terms of both tumor surface area and tumor signal intensity, using this quick method that does not require further histologic analysis.
Figure 1. ID8 Murine Ovarian Cancer Cells Express RFP. (A) Phase image of ID8 cells. (B) Fluorescence image of ID8 cells. Please click here to view a larger version of this figure.
Figure 2. Live Optical Imaging of C56/Bl6 Mouse with Intra-peritoneal Tumor Burden. (A) Depilatory cream was used to remove hair from the ventral surface of the mouse prior to scanning. (B) Diagram showing initial ventral midline and lateral incisions. Please click here to view a larger version of this figure.
Figure 3. Endpoint Scanning of Intra-Peritoneal Tumor Burden. (A, B) Mice are first imaged with organs in situ (ventral side down) following opening of the ventral surface of the mouse. (C,D) Imaging of individual organs. Each organ is dissected, visual tumor burden recorded, and placed on the organ scanning template for analysis. Please click here to view a larger version of this figure.
Figure 4. Organ Scanning Template. Dissected organs are placed on the organ scanning template to maintain positional identification of individual organs during scanning.
Figure 5. Normalized Quantitative Data for the Omentum/Pancreas, Ovaries and Mesentery. Data were analyzed as described in Protocol and as shown in Table 1. Mouse A refers to the mouse scanned in panel 3A; mouse B refers to the mouse scanned in panel 3B. (A) Normalized tumor area. Fluorescence signal quantification analysis of these three organs was conducted and quantified in terms of a ratio of tumor surface area to whole organ surface area for both mice. (B) Normalized raw integrated density. Fluorescence signal quantification analysis of these three organs was conducted and quantified in terms of a ratio of raw integrated density to whole organ surface area for both mice.
Omentum/Pancreas | |||
Normalized Tumor Area | Normalized Raw Integrated Density | ||
Mouse A | 0.5346 | 5.11E+07 | |
Mouse B | 0.0203 | 8.97E+05 | |
Ovaries | |||
Normalized Tumor Area | Normalized Raw Integrated Density | ||
Mouse A | 4.79E+07 | ||
Mouse B | 0.0123 | 5.62E+05 | |
Mesentery | |||
Normalized Tumor Area | Normalized Raw Integrated Density | ||
Mouse A | 0.2951 | 2.22E+07 | |
Mouse B | 0.0098 | 4.15E+05 |
Table 1. Normalized Tumor Area and Normalized Raw Integrated Density values in the Omentum/Pancreas, Ovaries and Mesentery of both Mouse A and Mouse B. Post dissection and scanning, each organ was segmented and its fluorescence quantified to determine the proportion of tumor area to total organ surface area and the intensities of the fluorescence for these tumor areas. The omentum/pancreas, ovaries and mesentery were selected as they had the strongest fluorescence signals within both the positive and negative control groups.
In contrast to studies using human ovarian cancer cells that must be conducted in immunocompromised mice, the protocol described above utilizes immunocompetent C57/Bl6 mice and syngeneic murine ovarian cancer cells. While this enables assessment of the potential role of immune infiltrates in tumor progression and metastasis, the presence of dark hair on the abdominal surface renders imaging less sensitive. Use of a depilatory to remove hair prior to imaging enhances image acquisition, but is time-consuming, particularly for experiments requiring longitudinal imaging. Hairless 'nude' mice can be used in this protocol and do not require depilatory-based hair removal. Furthermore, nude mice lack a functioning immune system, so can also be utilized to assess the growth of human ovarian cancer cells in experiments wherein the contribution of the immune system is not under analysis.
It should also be noted that the depth of intraperitoneal tumors also presents technical challenges, as optical fluorescence imaging will generally not detect tumors at depths greater than 5 mm. Furthermore, the prevalence of ascites fluid and the presence of ascitic tumor cells provide additional complications. We have observed significant mouse-to-mouse variability in the formation of ascites fluid, even when injected with the same cell line. Thus in the presence of ascites, this method is preferable for end-point analysis of organ-specific tumor burden rather than routine longitudinal imaging of progression. In the current case, dramatic changes in tumor burden were noted between the example mice, such that cohorts of four to five mice will usually be sufficient for statistical analysis. In the case of less dramatic differences in tumor burden, additional experimental subjects will be needed to reach statistical power. While the examples shown herein differ significantly in tumor volume, optical fluorescence imaging can be used to detect much smaller differences in organ-specific tumor burden, particularly when compared to weight- or caliper-based measurements on small lesions (not shown).Resolution and sensitivity will vary with cell line and imaging system. In the present case, metastatic implants as small as 400 µm in diameter can be resolved and quantified. Alternative methods including contrast-enhanced computed tomography (CT), magnetic resonance (MR) imaging, and positron emission tomography (PET) have been described for longitudinal imaging14,15. Modalities including combined anatomic and functional imaging are also under development16.
In regards to this proposed method for quantification of tumor burden, it should be noted that the determination of the fluorescence thresholds [Step 4.3.5.] is based on the intensity of the fluorescence seen in the organ images [Step 4.3.2.] and is chosen by the user to include only the most fluorescent regions relative to the rest of the organ. Varying threshold values were used in the analysis before determining the final threshold values used in this study. Once determined, these same thresholds were used for every organ analyzed so as to ensure consistency in the quantification of what is deemed metastatic tissue by the initial visual analysis done by the researcher. The determination of these thresholds is a critical step in the procedure and potentially could vary from one project to the other as determined by the individual researcher. In this case, a large lower threshold was used so as to capture only the highest intensity fluorescence signals. By using this same threshold for every organ analyzed, the analysis and results offer comparative quantitative results within the context of this cohort of mice. While this method is limited in quantification of absolute values of tumor surface area, it allows researchers the ability to compare relative normalized tumor burden among the same and different organs within cohorts of mice. It should be noted that this approach includes quantification of tumors that are not visible to the naked eye.
The unique metastatic mechanism of EOC results in widely disseminated intraperitoneal carcinomatosis involving multiple tissues and organs, rendering optimal cytoreductive surgery technically challenging. As complete cytoreduction positively correlates with overall survival, it follows that the development of new therapeutic strategies to combat intra-peritoneal metastasis is warranted. Assessment of therapeutic efficacy, however, is dependent on accurate quantitation of tumor burden, including evaluation of organ-specific metastasis. Using optical imaging of RFP-tagged tumor cells in situ corrected for organ autofluorescence, combined with careful ex vivo organ imaging, we have developed an approach to quantify intraperitoneal organ-specific tumor burden. Interestingly, our analyses show that preferred sites of metastasis in this model, as defined by tumor burden/surface area, are similar to those found in women with ovarian cancer (omentum, ovary, intestine, mesentery)2,4,5. Therefore this approach should have future utility in evaluation of experimental therapeutics designed to target metastatic disease.
The authors have nothing to disclose.
This research was supported by research grants RO1CA109545 and RO1CA086984 to M.S.S. by the National Institutes of Health/National Cancer Institute and by an award from the Leo and Ann Albert Charitable Trust (to M.S.S.).
Dulbecco's Modified Eagle Medium | Corning | 10-014-CM | |
Fetal bovine serum | Gibco | 10437-028 | |
penicillin/streptomycin | |||
Insulin-transferrin-sodium selenite media supplement | Sigma | I-1884 | |
Bruker Xtreme small animal imaging system | Bruker Corp. | ||
Bruker Multispectral software | Bruker Corp | ||
lentiviral particles with Red fluorescent protein | GenTarget, Inc. | LVP023 | |
trypsin for cell culture | Corning | 25-053-CI | |
PBS | Corning | 21-040-CM | |
depilatory cream (such as Nair Hair Remover Lotion) | purchases from drugstore | n/a | |
ImageJ software | http://imagej.nih.gov/ij/ | free download | |
dissecting tools (forceps) | Roboz Surgical Instrument | RS 5130 | |
dissecting tools (Scissors) | Roboz Surgical Instrument | RS 5910 |