Considerations in the development of circulating tumor cell technology for clinical use
Journal of Translational Medicine volume 10, Article number: 138 (2012)
This manuscript summarizes current thinking on the value and promise of evolving circulating tumor cell (CTC) technologies for cancer patient diagnosis, prognosis, and response to therapy, as well as accelerating oncologic drug development. Moving forward requires the application of the classic steps in biomarker development–analytical and clinical validation and clinical qualification for specific contexts of use. To that end, this review describes methods for interactive comparisons of proprietary new technologies, clinical trial designs, a clinical validation qualification strategy, and an approach for effectively carrying out this work through a public-private partnership that includes test developers, drug developers, clinical trialists, the US Food & Drug Administration (FDA) and the US National Cancer Institute (NCI).
The Foundation for the National Institutes of Health (FNIH) Biomarkers Consortium is a public-private biomedical research partnership that promotes the development and qualification of promising biomarkers for the prevention, early detection, diagnosis and treatment of disease. Consortium partners include patient advocates, clinical researchers from academia and industry, industry members from both therapeutic and diagnostic industries, the NCI, and the FDA. The Cancer Steering Committee (CSC) of the Biomarker Consortium focuses specifically on research activities to further improve treatment for patients with cancer through the use of biomarkers in drug development and in the field of personalized medicine. To this end, the CSC is currently sponsoring several imaging and other cancer biomarker studies.
A particular goal of the CSC is to identify new technologies with the potential to contribute to biologically informed drug development and clinical medicine. One such area is the emerging field of CTC detection and analysis. The potential implications of successful development of appropriate technologies are very large, and exciting new technologies are under development. However, many questions remain unanswered regarding the biology of CTCs, how best to enumerate and characterize them and the path to regulatory and general clinical acceptance for technology platforms currently under development.
Because of its composition and the skill sets and activities of its member organizations, the Biomarkers Consortium is uniquely positioned to help answer some of these important questions. To this end, the Consortium sponsored a workshop on qualification and validation of CTC assays. This paper summarizes not only the discussions from that meeting, but the outcome of a series of further deliberations by a CTC Working Group (CWG) convened by the CSC. The results will be the basis of a series of clinical studies to be conducted by the CSC to help answer these CTC questions, and move the field forward.
CTCs: A background
CTCs have been defined as cancer cells of solid tumor origin found in the peripheral blood. It is generally thought that these cells detach from primary or secondary tumors of patients with advanced cancer prior to detection in the circulation. CTCs are considered very rare, with an estimated frequency of one in 100 million to one in a billion blood cells[1, 2]. CTCs have been detected in the peripheral blood of patients with advanced stages of most types of solid tumor cancers, and their presence may represent the hematogenous phase of metastasis since CTCs are often not seen until tumors have achieved neovascularization[1, 3]. However, CTCs have also been detected in the peripheral blood of patients with localized cancers, which may be indicative of increased risk of progression to metastatic disease[4–10], and very early during tumor development, even at a pre-malignant stage in a pancreatic cancer model.
Certain phenotypic characteristics have been utilized consistently to identify CTCs in the peripheral blood. CTCs were initially characterized as non-leukocytic, nucleated cells that are typically epithelial in origin, and maintain significantly larger diameters and total membrane surface areas than normal blood cells. However, the morphological features of CTCs are now known to be less clearly defined, and may vary by disease, disease stage (at the time of diagnosis), or disease state (e.g., pre- vs. post-treatment setting). In addition, a significant number of CTCs may lose their epithelial antigens and express the phenotypic markers of epithelial-mesenchymal transition (EMT), a phenotypic change that is thought to be an important feature in the metastatic process that allows tumor cells to travel to the site of metastasis formation without being affected by conventional treatment[12–15].
It is unknown if CTCs represent more aggressive cells than those in the tumor of origin. However, phenotypic assessments to date suggest that at least some subset of CTCs may represent viable metastatic precursor cells capable of initiating a clonal metastatic lesion[12–15]. In this context, the importance of tumor-stroma interactions in generation and/or maintenance of the cancer “stem”/tumorigenic cell status (tumor plasticity) should not be underestimated. The resulting molecular and phenotypical alterations are complex and may vary by cancer (sub) type, over time, and by stage of the disease (e.g.,). These complexities introduce additional challenges for interpreting CTC analysis results.
The analytical methods/assays used and the degree of their validation will be critical to establishing a common set of criteria describing CTCs. Progress in use of different CTC-related platforms for specific applications in the clinic (beyond CTC enumeration being monitored at multiple time points during the course of patient’s treatment) depends on establishing such criteria, keeping in mind how well the malignant features of detectable circulating cells are defined, and in the context of other molecular findings, to what extent identified CTCs could be helpful in detecting emerging resistance to treatment. This latter aspect could be critical for early modification of therapy, thus contributing to personalized health care.
A recent insight derived from CTC analyses has involved finding clusters of CTCs in the circulation of patients with advanced cancer[17–19]. It is not clear whether these aggregates are artifacts of sample processing, or if the detection of clusters has previously been limited by the technologies used for CTC isolation, most of which are purification approaches likely to disrupt clusters. Early studies suggest that CTC clusters may be relatively protected from cell death and the harsh environment and shear stresses of the vascular circulation; they may also be clinically significant; particularly the number, size, or composition of the clusters[17–19, 21–23]. The presence of clusters may be a better biomarker for increased metastatic potential than single CTCs[17, 18, 22].
Major questions to be answered concerning CTCs
The phenotype(s) of CTCs has not been fully defined. It is currently accepted that CTCs are morphologically EpCAM+, cytokeratin (CK)+, and CD45−. However, there is evidence that these cells can also occur in patients with benign diseases of the colon and other phenotypes may be present in the blood of metastatic cancer patients, including CD45+, CK + cells. It has been shown that these double-positive cells can be the result of long storage, and probably represent artifacts (which is consistent with evidence that that CK +, CD45 + cells do not have prognostic impact). Further, while CTCs are thought to seed metastatic sites from a primary tumor, there is known discordance between tumor tissue biomarker expression and CTC biomarker expression, as well as heterogeneity of biomarker expression among multiple metastatic sites[26–28]. This suggests that CTCs from metastatic sites can in themselves seed new sites (e.g.,). In addition, recent studies have shown that CTC markers may change over the course of therapy (e.g.,).
Identification of predictive biomarkers in CTCs has the potential to become a breakthrough in cancer diagnostics and drug development. There are many sensitive and reliable tools that may be used for the characterization of CTCs, including immunocytochemistry, immunofluorescence, laser scanning, fluorescence in situ hybridization (FISH), and polymerase chain reaction (PCR) techniques[9, 31–33]. However, statistically meaningful numbers of CTCs may need to be isolated in order to characterize the heterogeneity, determine cellular origin (primary vs. metastatic tumor), and evaluate CTC response (signalling, proliferation, and apoptosis) after therapeutic interventions. Through initiatives such as the NCI Alliance in Nanotechnology in Cancer, Clinical Tumor Proteomics Analysis Consortium, The Cancer Genome Atlas, and the Physical Sciences in Oncology Centers, the NCI Center for Strategic Scientific Initiatives (CSSI) is contributing to this effort by providing the community with large-scale, reproducible genomic, epigenomic, and proteomic signatures, and with advanced, robust technologies to examine such signatures at high-throughput and high-resolution.
The biomarker development process and development of CTCs as biomarkers
Validated CTC assays and CTCs qualified as biomarkers of cancer prognosis and response to therapy through the FDA Center for Drug Evaluation (CDER) process have the potential to improve the diagnosis and care of cancer patients, one of the goals of personalized medicine. The FDA defines a validated biomarker assay as an analytical test system with well-established performance characteristics and for which there is an established scientific framework or body of evidence that elucidates the physiologic, toxicological, pharmacologic, or clinical significance of the test results. For qualification, the results of biomarker measurements are expected to have met evidentiary standards within specific contexts of use linking the biomarker result with clinical measurements, and to be reliable for specific interpretations and applications in drug development and clinical and regulatory decision-making.
There are several ways by which biomarkers gain acceptance for regulatory decision making through the FDA. On a case-by-case basis, data on candidate biomarkers that are either used to make decisions in clinical trials or are being considered as a biomarker in human safety studies may be submitted to an investigational new drug application (IND), new drug application (NDA), or biologics license application (BLA). Alternatively, a test for a biomarker that will be required to support the dose selection, safety, or effectiveness of a drug, and that a sponsor will thus integrate into the drug development program, may be submitted as part of a co-development of drug and test combination (i.e., as a companion diagnostic).
Finally, FDA CDER has developed a Biomarker Qualification program as an outgrowth of the Critical Path Initiative to capture consensus on the context of use and supporting data for biomarkers, and to encourage the development of new biomarkers. Through this program, biomarker qualification is defined as “a conclusion that within a carefully and specifically stated ‘context of use’, the biomarker has been demonstrated to reliably support a specified manner of interpretation and application in drug development”. Once qualified, biomarkers can be used in the qualified context in INDs, NDAs, and BLAs; CDER regulatory reviews in all offices and disciplines will adhere to the qualification decision. However, an in vitro diagnostic device, e.g., a CTC test, needed to measure a qualified biomarker is required to be cleared by the FDA Center for Devices and Radiological Health (CDRH) with data supporting the analytical and clinical performance if it is to be used clinically as a diagnostic test, i.e., to inform patient management.
The voluntary process of qualification is intended for biomarkers that will be used as drug development tools. Since public knowledge and access are often essential to the process, collaborative groups such as the Biomarkers Consortium can be useful sources of candidate biomarkers. The process itself provides a framework for interactions between CDER (and often other centers within FDA) and sponsors, with CDER guidance towards the compilation of comprehensive evidence to support the end result of qualification. The interactions include initial evaluation, interactive consultation and advice, and final in-depth review.
An analytically validated assay for the biomarker is a prerequisite for qualification, since the stability, accuracy, and reproducibility of the measurement will be critical to demonstrating utility. Candidate CTC-based biomarkers include the number and/or molecular sub-classification of target cells, and among the assays of interest are those that measure these parameters. Criteria for assessing the analytical validity of clinical assays have been published by the Clinical and Laboratory Standards Institute (CLSI), FDA’s Office of In Vitro Diagnostics, and other groups. Some considerations for evaluating the analytical and clinical validity of CTC assays are listed below, and reliability of data sources for determining clinical validity are listed in Table1.
CTC assay analytical validation considerations include the following:
Pre-analytic Variables Controlled
Materials at study site, e.g., sample collection tubes, shipping containers
Materials at analytic laboratory, e.g., assay-specific kit (w/instructions for use, reagents, buffers, controls, etc.), additional equipment (centrifuge, test tubes, micropipettes, vortex mixer, etc.)
Reagent storage conditions (temperature, time, etc.)
Specimen collection, e.g., timing of specimen collection relative to study treatments and procedures, phlebotomy procedure (patient positioning, needle size, blood draw site, sample size and number of samples, collection tube, tube inversion for clot prevention)
Specimen handling e.g., storage time and temperature, shipping time, etc.
Analytic Variables Controlled
Type of analysis (enrichment/enumeration/molecular characterization of target cells)
What is the range of specimens tested?
Sensitivity of assay (enrichment/enumeration/molecular characterization of all cells)
Specificity of assay (enrichment/enumeration/molecular characterization of only target cells)
How often does the assay give a useable result?
How similar are the results with repeated measurements?
What are the analytical range, reproducibility, and clinical applicability of the test?
How similar are the results obtained within the same or in multiple laboratories using the same or different technology?
Assay-specific controls should be run each day of analysis or when a new assay lot is used to check overall performance, including instrument, reagents, and operator technique
Assay-specific controls should be run regularly (monthly or quarterly) to show performance at the lower limit of analysis
Assay-specific samples should be run semi-annually to document the lower limit of quantitation
Calibration/calibration verification (at least semi-annually)
All participating laboratories in the same study should use common controls to document continuously across laboratory performance.
Splitting samples across laboratories prior to the study is recommended to document assay performance across laboratories.
CTC assay clinical validity considerations include the following:
Clinical sensitivity and specificity of assay
Are there methods to resolve clinical false positive assay results in a timely manner?
Prevalence (how often are the target cells detectable in the study population?)
What is the relationship between detectable target cells and the study disease?
Positive predictive value (what is the probability that a positive assay result means that the subject has the target disease?)
What are the genetic, environmental, or other modifiers for detection of the target cells?
A working group formed at the NCI–European Organisation for Research and Treatment of Cancer (EORTC) First International Meeting on Cancer Diagnostics convened in Nyborg, Denmark, in July 2000 created a set of criteria for high quality reporting of biomarker studies. The guidelines evaluate study design, methods, and analyses; and provide suggestions for the types of data elements that should be reported. These guidelines will be useful in obtaining data for evaluating and comparing CTC assays.
During clinical validation prospective clinical studies may be designed to show evidence of the link between the biomarker being measured and the specific biologic process or clinical outcome. Sometimes, links between a candidate biomarker and a biologic process or clinical outcome can be supported by examining retrospectively collected data or specimens for which the process or outcome in question is known, but this will generally provide only exploratory information that will need prospective confirmation. Retrospective collections of samples are not expected to contain stable/viable/molecularly unaltered CTCs, due to the labile nature of live cells once removed from the body.
Potential contexts of use for CTCs
Many potential clinical contexts of use exist for CTCs. Detection of CTCs may potentially be used to establish a diagnosis, as an alternative to invasive biopsies for early detection of metastatic tumor tissue, and for monitoring cancer patients[21, 38–40]. CTCs also have potential for investigation of heterogeneity in biomarker expression between primary tumors and distant metastases, as well as among multiple metastatic sites[9, 26–28, 30, 41]. Particularly interesting to the Biomarkers Consortium, the numbers and characteristics of CTCs may be prognostic for survival or predictive of response to cancer therapy in general or of response to a specific therapy. Moreover, changes in CTCs during the course of therapy may serve as biomarkers of treatment response or resistance.
Assays that enumerate or report the number of CTCs in a whole blood sample of a patient with advanced cancer have been shown to be prognostic for survival[42–44]. CTC enumeration via the Veridex CellSearchTM System is FDA-cleared for use as an aid in monitoring patients with metastatic breast, colorectal, and prostate cancers (FDA, CDRH). The presence prior to treatment of ≥5 CTCs in a 7.5 ml sample for metastatic breast and prostate cancers, and ≥3 CTCs for colorectal cancer is associated with decreased progression-free and overall survival, and is prognostic, regardless of therapy used. Recent studies have also shown the potential utility of the CellSearchTM assay for monitoring patients with melanoma, urothelial, and lung cancer[45–48].
Beyond enumeration, molecular profiling of CTCs has the potential to provide predictive information to guide the selection of therapy[49, 50]. For example, although several studies have not seen this correlation[9, 41, 50], other studies indicate that there is concordance for human epidermal growth factor receptor 2 (HER2) gene status between primary breast cancer tumors and CTCs. This suggests that targeting patients with HER2-positive (HER2+) CTC test results with the anti-HER2 antibody trastuzumab may significantly improve clinical outcomes for HER2+ breast cancer (e.g.,). CTC characterization may also aid in accelerating drug development and approval, since the focus of many current oncology drug discovery efforts is developing targeted therapies against signalling proteins implicated as important drivers of aggressive tumor growth and survival. A key step in the successful clinical development of such agents is the identification of responsive or resistant patient populations with predictive biomarkers for these therapies. The study of detailed molecular signatures for individual CTCs may also provide leads in new drug discovery by assessing the markers unique to progression so that relapsing patients can be treated for their current “molecular disease”.
As cancer cells can be more frequently sampled in circulation than through tumor biopsy, characterization of CTCs over time can provide an opportunity to better assess dynamic physiologic responses to treatment. Measuring CTCs sequentially during the course of therapy may reveal tumor evolution under therapeutic “natural selection” and permit the identification of biologic determinants of drug resistance or progression (e.g., secondary mutations)[9, 52, 53]. In this regard, evolutionary biologists working with the NCI Office of Physical Sciences-Oncology, are discovering instantaneous and long-term responses in more than 150 patients by examining robust data generated by high-content CTC platforms using ~2500 samples collected at regular timed intervals.
Post-therapy changes in CTCs might be an easily accessible intermediate point-of-response efficacy. Further, a number of cases have shown that CTC numbers change prior to changes being seen with anatomical imaging, and that CTC analysis may be a more robust surrogate of survival than anatomical imaging; so CTCs potentially may have more utility in the clinical setting[9, 10, 54]. CTC evaluation might ultimately be used as a surrogate measurement of clinical benefit and therefore an endpoint in clinical research.
A major challenge in processing and analyzing CTCs is their low concentration in blood. For example, detailed standard protocols for controlling pre-analytic variables associated with collection and handling of blood samples are likely needed to ensure reproducibility of assay results (see below under Standards). A wide range of assay platforms is currently under development for analysis of CTCs[29, 32, 50, 55]; the developers seek to optimize both sensitivity and specificity for detecting CTCs and to avoid generation of artifacts from extensive processing. Whole blood sample enrichment for CTCs generally involves density gradient centrifugation, immunomagnetic isolation, microfluidics, or some combination of techniques. CTC enumeration platforms are generally image-based approaches using immunocytochemistry or laser scanning cytometry, and CTC characterization techniques are typically nucleic acid or protein-based molecular assays, imaging, or a combination of molecular and imaging methods. As suggested by the background discussion above, each assay platform will likely have strengths and weaknesses in evaluating various aspects of CTCs. For instance, assays using immunomagnetics with anti-EpCAM antibodies are very efficient at enriching for epithelial cells but may miss cancer cells that have undergone EMT.
A number of promising techniques reported in the past few years use microfluidic devices to isolate CTCs from whole blood. In addition to enabling detection of CTCs in small blood samples, key design features of these techniques are flow patterns to optimize exposure of blood cells to the CTC detection method (often anti-EpCAM antibodies) and to minimize nonspecific leukocyte binding, as well as provision of platforms for molecular characterization of the captured cells. For example, among the microfluidics-based devices is one in which blood is pumped across a silicon-etched chip containing thousands of microposts fitted with anti-EpCAM antibodies. EpCAM-positive cells attach to the microposts and are then analyzed using dyes and imaging. An enhanced version of this CTC Chip uses microvortices in a herringbone pattern to increase the number of interactions between CTCs and the antibody-coated chip surface; DNA from cells captured on the chip are extracted and analyzed for specific molecular targets. Another microfluidics device contains sinusoidal micro channels coated with anti-EpCAM antibodies to capture CTCs; the captured cells are detached from the micro channels using trypsin and passed through a conductivity sensor on the device for enumeration. Specific to prostate cancer, a microfluidic device with a three-dimensional flow pattern has been described that uses anti-prostate specific membrane antigen (PSMA) antibody to capture CTCs (PSMA+, CD45− cells). Captured cells are fixed on the device and stained for PSMA, EpCAM, and presence of a nucleus; CTCs are enumerated with the aid of confocal microscopy. The captured cells can be made permeable to enable detection of intracellular antigens (e.g., TMPRSS-ERG fusion protein) or lyzed for RNA extraction. Table2 lists some of the more widely publicized CTC assays and assay platforms being developed for commercial use, including those with microfluidic and microarray technology.
Selection of CTC technologies for clinical development
One of the goals of the Biomarkers Consortium Workshop was to bring together experts in the field of CTC research to identify and implement practical ways of comparing the performance of the most promising CTC assay technologies at equivalent levels of development as an initial step in clinical validation. This work, viewed as a preliminary step, was necessary to determine the value of a particular technology for inclusion in clinical trials. Discussions from the workshop and recommendations from subsequent CWG meetings are summarized below.
Selected CTC assays could range from relatively low technology immunoassays for enumeration to more advanced technology platforms for molecular analysis, but priority should be given to examination of technologies with robust analytical validation and potential for providing data to address the key questions regarding biology and clinical significance of CTCs.
Clearly, different technologies may be more or less appropriate for specific applications, and more than one assay may be required for different contexts of use in a given patient. For example, a technology optimized for enumeration might not be optimal for providing enriched or purified CTC populations for detailed biological characterization. Therefore, no simple generalization can be made about the “ideal CTC technology”. Nevertheless, general comments can be made regarding characteristics which each technology should possess.
For example, the CTC technologies selected for evaluation should be ready to use in a clinical laboratory setting (see Table3). Standard reference materials for the assay should be available and readily accessible by laboratories involved in clinical studies, and standards should be in the clinically informative range (able to show that quantitation or other analysis is accurate and reproducible at the cut-off level). As noted above, the assays selected should already have published performance data with a known performance at the level that is appropriate for use in clinical trials; depending on the technology, there should also be independent analytical validation for different organ systems. The effects of pre-analytical variables related to biospecimen acquisition, processing, and transportation should be predetermined for each assay type and serve as the evidence base for standardized procedures to obtain and handle assay samples. Each assay should demonstrate a relevant dynamic range in response; where appropriate, the assay should provide capabilities for identifying biologically relevant point mutations and ideally capture viable cells for additional analyses. Each testing laboratory needs to validate the assay using the manufacturer’s published data as guidance in developing internal validation criteria.
Workshop participants and the CWG strongly endorsed the development of standard language for describing CTCs and of standard operating procedures (SOPs) for clinical evaluation of CTC assays prior to any testing on patient specimens. For example, different CTC subtypes may need to be defined, and the definitions should be context-dependent. Creating a panel of criteria for describing CTCs that together can provide statistical confidence provides an alternative approach.
Pre-analytic protocol standards for acquiring, handling, and transporting samples, and acquiring, processing, and interpreting assays are needed to allow collaboration among centers at a level of detail sufficient to encompass all likely variables. These standards should enable comparisons across platforms, contexts of use, and time. Efforts should be made to develop protocols for evaluating technologies that are uniform and clinically meaningful with regard to well-defined parameters for specific applications. Though ideally flexible enough so that new technologies can be easily integrated, the standards should be evaluated rigorously.
While specific procedures for sample acquisition, handling, and processing should probably be dictated by the analysis to be done, general recommendations for sample handling should be made. Pre-analytical variables, including fasting status, time of day, body positioning during the blood draw, and venipuncture needle size should be standardized. It also may be desirable for CTC assay platform companies to supply completely self-contained collection kits to minimize the pre-analytic variability. Procedures for handling acquired samples, including sample transport and storage, should also be standardized and deviations tracked variables related to sample collection and analysis are listed following:
Materials at Site
Sample collection kit with instructions for use
Temperature monitoring strips
Materials at Lab
Appropriate analytical instrumentation
Multiple levels of controls
Reagent storage temperature
Reagent storage time
Patient preparation—for example, fasting status
Sample Collection Variables
Timing of sample collection in study protocol
Sample collection method
Number of specimen collected, including duplicates
Subject positioning during sample collection
Specimen transport time
Specimen storage temperature
Specimen storage time
Lot-specific control testing
Levels of quality control testing (daily, monthly)
Assay platform training
All testing should use rigorous criteria such as Clinical Laboratory Improvement Amendments (CLIA) or good laboratory practice (GLP) standards. Early-stage development studies of clinical assays are not subject to CLIA regulation; however, clinical trials where biomarker assays are integral to the design need to be done in CLIA-certified laboratories, and if the results of the assay are used to make treatment decisions, FDA review is generally needed. Biomarker assays are considered to play an integral role when done in real time and the results used for trial eligibility or to make individual patient decisions—for example, to stratify patients, assign a patient to a specific treatment arm, or decide whether to escalate dose or stop treatment.
The fragility/lability of tumor cells introduces an important source of variability in the evaluation of CTC assay platforms that analyze captured whole cells, since CTC apoptosis begins very early after separation from the tumor of origin and after removal of blood from the patient[59–61]. Incorporating cellular preservatives in the collection of peripheral blood samples has been shown to stabilize CTCs for up to 96 hours[25, 32, 61]. Standard use of this procedure would allow greater flexibility in sample storage and shipping, which in turn may allow the inclusion of more enumeration assay technologies in comparison evaluations, and make their utilization in the clinic more practical.
Archived CTC samples may be adequate for molecular-based assays, assuming that one is able to demonstrate that the cells of interest have survived the archiving procedure and duration in numbers and biological condition that represent their state when collected. However, access to systematically collected and appropriately well-preserved patient samples with linked clinical outcome data is essential. For CTC studies in general, archived tumor samples may be difficult to obtain, suboptimal for certain molecular assays, or not representative of a patient’s disease at the time of treatment. The NCI has provided detailed recommendations related to biospecimen and data quality in the 2010 Revised NCI Best Practices. The NCI Office of Biorepositories and Biospecimen Research (OBBR) is one resource for well-defined archived samples that are collected using the most stringent SOPs.
Established in 2005, a goal of OBBR is to develop a common biorepository infrastructure to facilitate multi-institutional genomic and proteomic studies. Partnering with an organization like OBBR to develop CTC-specific SOPs, as well as a source of clinical samples for assay comparison studies, should be considered.
Initial interassay comparison on clinical samples
For most new CTC technologies reviewed, it was noted that too little systematically collected data were available to allow evaluation of potential clinical utility or to compare with other assays. Beyond analytical validity, foundational data on the individual assays are needed, such as frequency of detection in specific patient populations and consistency of the results in a given patient in determinations on multiple days and at different time intervals, as well as the capability for detecting quantifiable changes to a patient’s results after appropriate treatment.
Specificity of a CTC assay depends on a particular test result representing the target tumor cells, as opposed to normal hematopoietic or circulating epithelial cells. This distinction can often be made by either visual inspection by a trained cytopathologist or by determination of molecular markers, or a combination of these techniques. For example, Meng et al. have demonstrated that in patients with metastatic breast cancer, epithelial cells identified using an immunomagnetic separation system with anti-EpCAM as the capture antibody are highly aneusomic and almost certainly malignant and not normal. Further, Shaffer et al. demonstrated that cells captured by CellSearch™ expressed prostate specific antigens and had molecular features of malignancy as determined by FISH analysis.
However, it is conceivable that not all cells that meet visual or molecular criteria for cancer have true malignant potential or, conversely, that not all cells lacking the defined criteria are nonmalignant (e.g.,[24, 63]). Current thought is in part based on stem cell theory, which posits that only a fraction of any tumor mass, and therefore of any CTC population, is able to establish and maintain a metastasis. Also as suggested above, it is known that many cells identified in the circulation are already undergoing, or have completed, apoptosis. Therefore, biologic relevance is not just the presence of unequivocally malignant-appearing cells, but the biological and/or clinical significance of these cells. The latter can only be determined by correlating the presence of assay metrics (presumed CTCs) with some clinically or biologically important outcome, such as tumor regression, subsequent recurrence, new primary cancer, or death.
The implication of biologic significance is that one cannot conclude that a new assay is superior to a gold-standard assay by mere comparison of assay metrics/unit blood between the two. One must determine whether a presumably more sensitive assay retains, or exceeds, the robust separation of outcomes between patients who are positive vs. those who are negative for the assay, and this can only be demonstrated in well-designed clinical studies.
Direct comparison of different technologies on the same clinical samples and/or in tumor cell spiking experiments would be informative. One or two specific CTC-derived biomarkers (e.g., EpCAM) could be used to identify the optimal assay technologies. Gold-standard technologies are needed for comparisons, based on whether the evaluation is quantitative (enumeration of CTCs) or qualitative (molecular characterization of CTCs). CellSearch™ could serve as an anchor in the short term for assessments of newer enumeration assay technologies, building on prior clinical evidence for its predictive and prognostic capability.
The CWG discussed approaches to carry out this evaluation in which the Biomarkers Consortium would provide a framework wherein laboratories studying the selected technologies would have access to matched pre- and post-treatment clinical samples from multiple clinical settings as obtained by the OBBR or an equivalent source. The samples could be from patients treated with approved therapies (e.g., the control arms of randomized clinical trials), well-annotated regarding patient characteristics and outcomes, and collected and processed according to standard protocols as described above. Fresh blood samples may be needed for these studies since archived samples may contain degraded cells and no longer reflect the disease state of the donor at the time of collection. The samples could be analyzed by multiple methods, would be blinded to the analyzing laboratory, and results data would be compiled by the CWG prior to release back to the assay developer. This approach would yield information regarding whether different technologies are detecting different CTC populations and provide information for definitions of analytically valid biomarkers that may need to be established for these different populations.
Clinical trial design considerations
Despite the fact that research aimed at defining and understanding the biology of CTCs is still ongoing and many promising assays are still early in development, the Workshop participants and CWG believe that it is crucial to establish clinical validation and qualification trials soon with the goal of determining the true clinical relevance of CTCs and specific assays of CTCs. In this regard, the excellent on-going qualification work in collaboration with FDA regarding the use of CTCs as an efficacy response surrogate biomarker for survival in patients with advanced prostate cancer[38, 43] was acknowledged.
Beyond clinical validation of specific assays, CTC qualification studies should initially seek to answer clinically relevant questions, such as a) to determine the potential utility of CTCs in early clinical development of drugs (phase 1 and 2 trials); b) to determine if enumeration could be an early efficacy response marker; c) to help drive the use of enumeration as a surrogate marker of response to therapy; d) to investigate whether CTC evaluations could augment or replace imaging for response monitoring; and e) to investigate whether the molecular analysis of CTCs could replace tumor biopsies for patient stratification for targeted therapies. In the short term, there is general interest in the application of CTC enumeration for determining response to therapy; therefore, association of CTC measurements with complete response, partial response, stable disease, and progressive disease would be appropriate endpoints for initial clinical trials.
Several trial designs may be useful in addressing these questions regarding evaluation of clinical validity of CTC technologies and qualification of CTC measurements as biomarkers of response to therapy. First, CTC substudies may be added to ongoing trials where the study treatment choices and primary endpoints (early endpoints such as objective response, as well as clinical outcomes) would be dictated by the parent trial. Single-arm studies could be used to explore changes pre- and post-therapy and correlation with outcomes, thus assisting with determining cut points. As single-arm trials can only evaluate prognostic potential, two-arm, two-drug substudies could also be used to compare results with different therapies to evaluate the predictive potential of CTCs. Alternatively, the CTC study may be fully integrated into the trial design. In this design, patients would be randomized on the basis of the presence or absence of CTCs. The FDA has recommended this study design to evaluate diagnostic tests for use in the selection of drug therapy.
One example of an ongoing clinical trial to test the clinical utility of CTCs is SWOG S0500. In this trial, women starting a first line chemotherapeutic regimen for hormone-refractory metastatic breast cancer and who have persistently elevated CTCs after one cycle are randomly assigned to continue their therapy until classic evidence of progression (history, physical examination, imaging) or to change immediately to a different regimen. The goal of this study is to demonstrate an improved overall survival for women who are switched, based on a CTC test result (see Figure1), from an apparently ineffective treatment strategy to an alternative one. Patient populations where treatments have the potential to change based on the results of the trial should be targeted. The cohorts should include patients with measureable, advanced, non-hematologic cancers, as currently the most interesting and appropriate clinical application of CTC analysis is to establish its predictive value for response to therapy.
In terms of study indication, there should be no bias for target tumors other than the robustness of the available data. Robust CTC data have been obtained with the CellSearch™ System for breast, colorectal, and prostate disease. With the same technology, low numbers of CTCs are captured in the metastatic settings for colon and lung cancer; therefore, newer technologies with higher sensitivity and good specificity rates may be useful in these settings. In early disease, such as neoadjuvant settings, where fewer CTCs are expected[8, 9, 65], a potential benefit of more sensitive assays could be a shorter timeframe to analysis of study endpoints like the extent of residual disease after surgery as an early marker of outcome, which provides value for new drug development. In addition to more efficient enumeration, newer technologies provide the promise of molecular profiling of tumor response to therapy in all the clinical designs described.
A clinical validation and qualification study strategy and process
The CSC of the Biomarkers Consortium is interested in supporting a series of studies to help resolve important pre-competitive issues around CTCs, with the overall objectives of providing evidence toward qualification of CTC derived biomarkers for assessing prognosis pre-therapy, establishing CTC number as a surrogate for survival, and determining whether the molecular profile of CTCs predict response to treatment.
The initial goal of the proposed strategy will be to demonstrate the robustness of candidate CTC assay technologies currently under development, prior to clinical studies, in order to determine which of the platforms are closest to being ready for validation in the clinical trial setting. The proposed studies will evaluate newer CTC enumeration assays considered to be the most promising technologies using criteria created by the CSC and CWG against the FDA-cleared analytically valid CellSearch™ assay. The most promising CTC molecular characterization assays will also be compared using these criteria. Additionally, recognizing the need for standardizing procedures for specimen collection and processing to ensure the reliability of CTC measurements, the CWG will develop these procedures for CTC assays evaluated in this project. A small pilot in this regard was recently presented at an OBBR symposium, where CSSI, Offices of Physical Sciences-Oncology (OPSO), and OBBR are collaborating to examine the potential of using high-content systems to measure the effect of pre-analytical variables on biophysical parameters associated with biospecimens.
For cell spiking experiments, cell lines considered appropriate for the selected technologies will be obtained and cultured in standard conditions. Fluorescent labelling of target cells will be performed using standard cell labelling kits. Multiple samples from a given cell suspension will be counted and averaged to produce a mean cell count with a small standard deviation in order to minimize counting errors. The cell suspensions will then be appropriately diluted and processed using the selected CTC assay technologies. Capture efficiency percentages will be calculated using criteria as defined by the CWG.
In clinical studies, triplicate specimens will be collected from subjects participating in ongoing studies with relevant indications and study populations in order to compare the candidate assays against each other. For the CTC enumeration studies, one of each set of three samples will be analyzed using the CellSearch™ assay. Similarly, for the CTC molecular characterization studies, one assay will be selected to be used as the anchor. All clinical samples will be procured through the OBBR, or using SOPs compliant with OBBR requirements.
In the clinical validation studies, CTC substudies will be conducted in prospective phase 2 or 3 clinical trials (or if the assays selected do not require fresh blood, archived samples will be accessed from completed prospective studies for retrospective analysis) in an attempt to correlate CTC measurements with clinical outcomes related to treatment response, and time-related outcomes such as time to progression or disease-free survival. Here, duplicate specimens will be collected. The CTC assays will be performed pre-therapy and at defined intervals post-therapy on anonymized patient samples collected in the trial, blinding technicians to any patient identifiers. The specimens will be collected at participating sites and forwarded to the specified clinical laboratories for processing. In addition to SOPs for variables associated with sample collection as outlined above standard protocols are needed to allow comparison of CTC assay results across technology platforms. Just as challenging is the development of standards for collecting certain data points to analyze after advances have occurred in the field, so comparisons could be made over time. The standards would have to be flexible to easily incorporate new technologies.
After performing clinical validation studies, the next stage, qualification, would be follow-on clinical studies to determine the context-of-use of specific CTC measures. These studies will most likely be conducted in the phase 3 metastatic disease trial setting for specified indications in specified study populations. Baseline CTCs would be assessed, and then additional assessments would be made at some point after the start of treatment. These assessments may be used to determine the role of CTC analysis for monitoring disease recurrence, evaluating new treatments against standard therapy, or investigating concordance between imaging and CTC analysis. If a series of studies with clinical benefit outcomes shows good correlation and reproducibility between a given CTC measure and survival, that biomarker could be considered a candidate for FDA qualification.
Without question, the Veridex CellSearch™ assay and the advanced technologies now being applied to CTC detection and analysis have high promise for providing biomarkers and biomarker assays useful in oncological drug development, monitoring the course of disease in cancer patients, and in understanding the biology of cancer progression. However, many questions remain unanswered regarding the biology of CTCs, best methods for their enumeration and characterization, and the path to regulatory and general clinical acceptance for technologies currently under development. Standard protocols for acquisition and processing of blood samples, as well as sources of well-annotated clinical samples (including clinical outcomes) and application of criteria for analytical and clinical validation of CTC assays and qualification of CTC-based biomarkers are mandatory for the next steps in evaluation of these technologies. Developing and applying these standards is difficult, if not impossible, for individual research institutions and companies; this effort requires coordinated clinical trial resources for obtaining samples and infrastructure for developing standards, managing the collection and distribution of samples, and evaluation of test results, as well as input from engaged scientists and the FDA. To this end, the Biomarkers Consortium, as a public-private partnership, is proposing and planning to implement the framework described in this review.
As noted above, each author contributed direct experience in the development of drugs or biomarkers, development and application of CTC technologies, or both.
Biologics license application
Center for Drug Evaluation and Research
Center for Devices and Radiological Health
Clinical laboratory improvement amendments
Clinical and Laboratory Standards Institute
Cancer Steering Committee
NCI Center for Strategic Scientific Initiatives
Circulating tumor cell
CTC working group
Dielectrophoretic field flow fractionation
European Organisation for Research and Treatment of Cancer
US Food & Drug Administration
Fluorescence in situ hybridization
Foundation for the National Institutes of Health
Functionalized structured medical wire
Good laboratory practice
Human epidermal growth factor receptor 2
Investigational new drug application
US National Cancer Institute
New drug application
NCI Office of Biorepositories and Biospecimen Research
NCI Office of Physical Sciences-Oncology
Polymerase chain reaction
Prostate specific membrane antigen
Reverse transcriptase-polymerase chain reaction
Standard operating procedures.
Yu M, Stott S, Toner M, Maheswaran S, Haber DA: Circulating tumor cells: approaches to isolation and characterization. J Cell Biol. 2011, 192: 373-382. 10.1083/jcb.201010021.
Nelson NJ: Circulating tumor cells: will they be clinically useful?. J Natl Cancer Inst. 2010, 102: 146-148. 10.1093/jnci/djq016.
Hou JM, Krebs M, Ward T, Morris K, Sloane R, Blackhall F, Dive C: Circulating tumor cells, enumeration and beyond. Cancers. 2010, 2: 1236-1250. 10.3390/cancers2021236.
Nagrath S, Stott SL, Lee RJ, Yu M, Ulkus LL, Iafrate JA, Smith MR, Tompkins RG, Sequist LV, Haber DA, Maheswaran S, Toner M: Detection and characterization of circulating tumor cells in localized and metastatic prostate cancer patients using CTC-Chip microfluidic technology. Proc Am Assoc Cancer Res. 2010, 101st: abstr 1136-
Bertolin M, Pigozzo J, Koussis H, Ghiotto C, Valente S, Michieletto S, Magro C, Rossi E, Zamarchi R, Bozza F, Jirillo A, Chiarion-Sileni V, Amadori A: Circulating tumor cells detection and evaluation of their apoptotic status in patients with localized breast cancer before and after surgery. J Clin Oncol. 2011, 29 (suppl): abstr e21127-
Muller V, Stahmann N, Riethdorf S, Rau T, Zabel T, Goetz A, Janicke F, Pantel K: Circulating tumor cells in breast cancer: correlation to bone marrow micrometastases, heterogeneous response to systemic therapy and low proliferative activity. Clin Cancer Res. 2005, 11: 3678-3685. 10.1158/1078-0432.CCR-04-2469.
Nagrath S, Sequist LV, Maheswaran S, Bell DW, Irimia D, Ulkus L, Smith MR, Kwak EL, Digumarthy S, Muzikansky A, Ryan P, Balis UJ, Tompkins RG, Haber DA, Toner M: Isolation of rare circulating tumour cells in cancer patients by microchip technology. Nature. 2007, 450: 1235-1239. 10.1038/nature06385.
Pierga JY, Bidard FC, Mathiot C, Brain E, Delaloge S, Giachetti S, de Cremoux P, Salmon R, Vincent-Salomon A, Marty M: Circulating tumor cell detection predicts early metastatic relapse after neoadjuvant chemotherapy in large operable and locally advanced breast cancer in a phase II randomized trial. Clin Cancer Res. 2008, 14: 7004-7010. 10.1158/1078-0432.CCR-08-0030.
Riethdorf S, Muller V, Zhang L, Rau T, Loibl S, Komor M, Roller M, Huober J, Fehm T, Schrader I, Hilfrich J, Holms F, Tesch H, Eidtmann H, Untch M, von Minckwitz G, Pantel K: Detection and HER2 expression of circulating tumor cells: prospective monitoring in breast cancer patients treated in the neoadjuvant GeparQuattro trial. Clin Cancer Res. 2010, 16: 2634-2645. 10.1158/1078-0432.CCR-09-2042.
Xenidis N, Ignatiadis M, Apostolaki S, Perraki M, Kalbakis K, Agelaki S, Stathopoulos EN, Chlouverakis G, Lianidou E, Kakolyris S, Georgoulias V, Mavroudis D: Cytokeratin-19 mRNA-positive circulating tumor cells after adjuvant chemotherapy in patients with early breast cancer. J Clin Oncol. 2009, 27: 2177-2184. 10.1200/JCO.2008.18.0497.
Rhim AD, Mirek ET, Aiello NM, Maitra A, Bailey JM, McAllister F, Reichert M, Beatty GL, Rustgi AK, Vonderheide RH, Leach SD, Stanger BZ: EMT and dissemination precede pancreatic tumor formation. Cell. 2012, 148: 349-361. 10.1016/j.cell.2011.11.025.
Aktas B, Tewes M, Fehm T, Hauch S, Kimmig R, Kasimir-Bauer S: Stem cell and epithelial-mesenchymal transition markers are frequently overexpressed in circulating tumor cells of metastatic breast cancer patients. Breast Cancer Res. 2009, 11: R46-10.1186/bcr2333.
Polyak K, Weinberg RA: Transitions between epithelial and mesenchymal states: acquisition of malignant and stem cell traits. Nat Rev Cancer. 2009, 9: 265-273. 10.1038/nrc2620.
Bednarz N, Eltze E, Semjonow A, Rink M, Andreas A, Mulder L, Hannemann J, Fisch M, Pantel K, Weier HU, Bielawski KP, Brandt B: BRCA1 loss preexisting in small subpopulations of prostate cancer is associated with advanced disease and metastatic spread to lymph nodes and peripheral blood. Clin Cancer Res. 2010, 16: 3340-3348. 10.1158/1078-0432.CCR-10-0150.
Joosse SA, Hannemann J, Spotter J, Bauche A, Andreas A, Muller V, Pantel K: Changes in keratin expression during metastatic progression of breast cancer: impact on the detection of circulating tumor cells. Clin Cancer Res. 2012, 18: 993-1003. 10.1158/1078-0432.CCR-11-2100.
Lilly B, Kennard S: Differential gene expression in a coculture model of angiogenesis reveals modulation of select pathways and a role for Notch signaling. Physiol Genomics. 2009, 36: 69-78.
Stott SL, Hsu CH, Tsukrov DI, Yu M, Miyamoto DT, Waltman BA, Rothenberg SM, Shah AM, Smas ME, Korir GK, Floyd FP, Gilman AJ, Lord JB, Winokur D, Springer S, Irimia D, Nagrath S, Sequist LV, Lee RJ, Isselbacher KJ, Maheswaran S, Haber DA: Toner M: Isolation of circulating tumor cells using a microvortex-generating herringbone-chip. Proc Natl Acad Sci U S A. 2010, 107: 18392-18397. 10.1073/pnas.1012539107.
Hou JM, Krebs M, Ward T, Sloane R, Priest L, Hughes A, Clack G, Ranson M, Blackhall F, Dive C: Circulating tumor cells as a window on metastasis biology in lung cancer. Am J Pathol. 2011, 178: 989-996. 10.1016/j.ajpath.2010.12.003.
Hou JM, Krebs MG, Lancashire L, Sloane R, Backen A, Swain RK, Priest LJ, Greystoke A, Zhou C, Morris K, Ward T, Blackhall FH, Dive C: Clinical significance and molecular characteristics of circulating tumor cells and circulating tumor microemboli in patients with small-cell lung cancer. J Clin Oncol. 2012, 30: 525-532. 10.1200/JCO.2010.33.3716.
Molnar B, Ladanyi A, Tanko L, Sreter L, Tulassay Z: Circulating tumor cell clusters in the peripheral blood of colorectal cancer patients. Clin Cancer Res. 2001, 7: 4080-4085.
Serrano Fernadez MJ, Alvarez Merino JC, Martinez Zubiaurre I, Fernandez Garcia A, Sanchez Rovira P, Lorente Acosta JA: Clinical relevance associated to the analysis of circulating tumor cells in patients with solid tumors. Clin Transl Oncol. 2009, 11: 668-659.
Wang ZP, Eisenberger MA, Carducci MA, Partin AW, Scher HI, Ts’o PO: Identification and characterization of circulating prostate carcinoma cells. Cancer. 2000, 88: 2787-2795. 10.1002/1097-0142(20000615)88:12<2787::AID-CNCR18>3.0.CO;2-2.
Glinsky VV, Glinsky GV, Glinskii OV, Huxley VH, Turk JR, Mossine VV, Deutscher SL, Pienta KJ, Quinn TP: Intravascular metastatic cancer cell homotypic aggregation at the sites of primary attachment to the endothelium. Cancer Res. 2003, 63: 3805-3811.
Pantel K, Deneve E, Nocca D, Coffy A, Vendrell JP, Maudelonde T, Riethdorf S, Alix-Panabieres C: Circulating epithelial cells in patients with benign colon diseases. Clin Chem. 2012, 58: 936-940. 10.1373/clinchem.2011.175570.
Riethdorf S, Fritsche H, Muller V, Rau T, Schindlbeck C, Rack B, Janni W, Coith C, Beck K, Janicke F, Jackson S, Gornet T, Cristofanilli M, Pantel K: Detection of circulating tumor cells in peripheral blood of patients with metastatic breast cancer: a validation study of the Cell Search system. Clin Cancer Res. 2007, 13: 920-928. 10.1158/1078-0432.CCR-06-1695.
Meng S, Tripathy D, Shete S, Ashfaq R, Haley B, Perkins S, Beitsch P, Khan A, Euhus D, Osborne C, Frenkel E, Hoover S, Leitch M, Clifford E, Vitetta E, Morrison L, Herlyn D, Terstappen LW, Fleming T, Fehm T, Tucker T, Lane N, Wang J, Uhr J: HER-2 gene amplification can be acquired as breast cancer progresses. Proc Natl Acad Sci U S A. 2004, 101: 9393-9398. 10.1073/pnas.0402993101.
Wulfing P, Borchard J, Buerger H, Heidl S, Zanker KS, Kiesel L, Brandt B: HER2-positive circulating tumor cells indicate poor clinical outcome in stage I to III breast cancer patients. Clin Cancer Res. 2006, 12: 1715-1720. 10.1158/1078-0432.CCR-05-2087.
Chang HJ, Han SW, Oh DY, Im SA, Jeon YK, Park IA, Han W, Noh DY, Bang YJ, Kim TY: Discordant human epidermal growth factor receptor 2 and hormone receptor status in primary and metastatic breast cancer and response to trastuzumab. Jpn J Clin Oncol. 2011, 41: 593-599. 10.1093/jjco/hyr020.
Alix-Panabieres C, Schwarzenbach H, Pantel K: Circulating tumor cells and circulating tumor DNA. Annu Rev Med. 2012, 63: 199-215. 10.1146/annurev-med-062310-094219.
Wang LH, Pfister TD, Parchment RE, Kummar S, Rubinstein L, Evrard YA, Gutierrez ME, Murgo AJ, Tomaszewski JE, Doroshow JH, Kinders RJ: Monitoring drug-induced gammaH2AX as a pharmacodynamic biomarker in individual circulating tumor cells. Clin Cancer Res. 2010, 16: 1073-1084. 10.1158/1078-0432.CCR-09-2799.
Maheswaran S, Haber DA: Circulating tumor cells: a window into cancer biology and metastasis. Curr Opin Genet Dev. 2010, 20: 96-99. 10.1016/j.gde.2009.12.002.
Lianidou ES, Markou A: Circulating tumor cells in breast cancer: detection systems, molecular characterization, and future challenges. Clin Chem. 2011, 57: 1242-1255. 10.1373/clinchem.2011.165068.
Ignatiadis M, Rothe F, Chaboteaux C, Durbecq V, Rouas G, Criscitiello C, Metallo J, Kheddoumi N, Singhal SK, Michiels S, Veys I, Rossari J, Larsimont D, Carly B, Pestrin M, Bessi S, Buxant F, Liebens F, Piccart M, Sotiriou C: HER2-positive circulating tumor cells in breast cancer. PLoS One. 2011, 6: e15624-10.1371/journal.pone.0015624.
US Food and Drug Administration: Guidance for Industry: Qualification Process for Drug Development Tools. Draft Guidance. 2010,http://www.fda.gov/downloads/Drugs/GuidanceComplianceRegulatoryInformation/Guidances/UCM230597.pdf,
US Food and Drug Administration: Guidance for Industry: Pharmacogenomic Data Submissions. 2005
US Food and Drug Administration: Draft Guidance for Industry and Food and Drug Administration Staff: In Vitro Companion Diagnostic Devices Draft Guidance. 2011,http://www.fda.gov/downloads/MedicalDevices/DeviceRegulationandGuidance/GuidanceDocuments/UCM262327.pdf,
McShane LM, Altman DG, Sauerbrei W, Taube SE, Gion M, Clark GM: Reporting recommendations for tumor marker prognostic studies (REMARK). J Natl Cancer Inst. 2005, 97: 1180-1184. 10.1093/jnci/dji237.
Shaffer DR, Leversha MA, Danila DC, Lin O, Gonzalez-Espinoza R, Gu B, Anand A, Smith K, Maslak P, Doyle GV, Terstappen LW, Lilja H, Heller G, Fleisher M, Scher HI: Circulating tumor cell analysis in patients with progressive castration-resistant prostate cancer. Clin Cancer Res. 2007, 13: 2023-2029. 10.1158/1078-0432.CCR-06-2701.
Serrano MJ, Sanchez-Rovira P, Delgado-Rodriguez M, Gaforio JJ: Detection of circulating tumor cells in the context of treatment: prognostic value in breast cancer. Cancer Biol Ther. 2009, 8: 671-675. 10.4161/cbt.8.8.7834.
Danila DC, Anand A, Sung CC, Heller G, Leversha MA, Cao L, Lilja H, Molina A, Sawyers CL, Fleisher M, Scher HI: TMPRSS2-ERG status in circulating tumor cells as a predictive biomarker of sensitivity in castration-resistant prostate cancer patients treated with abiraterone acetate. Eur Urol. 2011, 60: 897-904. 10.1016/j.eururo.2011.07.011.
Fehm T, Muller V, Aktas B, Janni W, Schneeweiss A, Stickeler E, Lattrich C, Lohberg CR, Solomayer E, Rack B, Riethdorf S, Klein C, Schindlbeck C, Brocker K, Kasimir-Bauer S, Wallwiener D, Pantel K: HER2 status of circulating tumor cells in patients with metastatic breast cancer: a prospective, multicenter trial. Breast Cancer Res Treat. 2010, 124: 403-412. 10.1007/s10549-010-1163-x.
Cristofanilli M, Budd GT, Ellis MJ, Stopeck A, Matera J, Miller MC, Reuben JM, Doyle GV, Allard WJ, Terstappen LW, Hayes DF: Circulating tumor cells, disease progression, and survival in metastatic breast cancer. N Engl J Med. 2004, 351: 781-791. 10.1056/NEJMoa040766.
de Bono JS, Scher HI, Montgomery RB, Parker C, Miller MC, Tissing H, Doyle GV, Terstappen LW, Pienta KJ, Raghavan D: Circulating tumor cells predict survival benefit from treatment in metastatic castration-resistant prostate cancer. Clin Cancer Res. 2008, 14: 6302-6309. 10.1158/1078-0432.CCR-08-0872.
Cohen SJ, Punt CJ, Iannotti N, Saidman BH, Sabbath KD, Gabrail NY, Picus J, Morse M, Mitchell E, Miller MC, Doyle GV, Tissing H, Terstappen LW, Meropol NJ: Relationship of circulating tumor cells to tumor response, progression-free survival, and overall survival in patients with metastatic colorectal cancer. J Clin Oncol. 2008, 26: 3213-3221. 10.1200/JCO.2007.15.8923.
Rink M, Chun FK, Dahlem R, Soave A, Minner S, Hansen J, Stoupiec M, Coith C, Kluth LA, Ahyai SA, Friedrich MG, Shariat SF, Fisch M, Pantel K, Riethdorf S: Prognostic role and HER2 expression of circulating tumor cells in peripheral blood of patients prior to radical cystectomy: a prospective study. Eur Urol. 2012, 61: 810-817. 10.1016/j.eururo.2012.01.017.
Naoe M, Ogawa Y, Morita J, Omori K, Takeshita K, Shichijyo T, Okumura T, Igarashi A, Yanaihara A, Iwamoto S, Fukagai T, Miyazaki A, Yoshida H: Detection of circulating urothelial cancer cells in the blood using the Cell Search System. Cancer. 2007, 109: 1439-1445. 10.1002/cncr.22543.
Okumura Y, Tanaka F, Yoneda K, Hashimoto M, Takuwa T, Kondo N, Hasegawa S: Circulating tumor cells in pulmonary venous blood of primary lung cancer patients. Ann Thorac Surg. 2009, 87: 1669-1675. 10.1016/j.athoracsur.2009.03.073.
Steen S, Nemunaitis J, Fisher T, Kuhn J: Circulating tumor cells in melanoma: a review of the literature and description of a novel technique. Proc (Bayl Univ Med Cent). 2008, 21: 127-132.
Gradilone A, Naso G, Raimondi C, Cortesi E, Gandini O, Vincenzi B, Saltarelli R, Chiapparino E, Spremberg F, Cristofanilli M, Frati L, Aglianò AM, Gazzaniga P: Circulating tumor cells (CTCs) in metastatic breast cancer (MBC): prognosis, drug resistance and phenotypic characterization. Ann Oncol. 2011, 22: 86-92. 10.1093/annonc/mdq323.
Pantel K, Brakenhoff RH, Brandt B: Detection, clinical relevance and specific biological properties of disseminating tumour cells. Nat Rev Cancer. 2008, 8: 329-340. 10.1038/nrc2375.
Meng S, Tripathy D, Shete S, Ashfaq R, Saboorian H, Haley B, Frenkel E, Euhus D, Leitch M, Osborne C, Clifford E, Perkins S, Beitsch P, Khan A, Morrison L, Herlyn D, Terstappen LW, Lane N, Wang J, Uhr J: uPAR and HER-2 gene status in individual breast cancer cells from blood and tissues. Proc Natl Acad Sci U S A. 2006, 103: 17361-17365. 10.1073/pnas.0608113103.
Maheswaran S, Sequist LV, Nagrath S, Ulkus L, Brannigan B, Collura CV, Inserra E, Diederichs S, Iafrate AJ, Bell DW, Digumarthy S, Muzikansky A, Irimia D, Settleman J, Tompkins RG, Lynch TJ, Toner M, Haber DA: Detection of mutations in EGFR in circulating lung-cancer cells. N Engl J Med. 2008, 359: 366-377. 10.1056/NEJMoa0800668.
Bidard FC, Mathiot C, Degeorges A, Etienne-Grimaldi MC, Delva R, Pivot X, Veyret C, Bergougnoux L, de Cremoux P, Milano G, Pierga JY: Clinical value of circulating endothelial cells and circulating tumor cells in metastatic breast cancer patients treated first line with bevacizumab and chemotherapy. Ann Oncol. 2010, 21: 1765-1771. 10.1093/annonc/mdq052.
Budd GT, Cristofanilli M, Ellis MJ, Stopeck A, Borden E, Miller MC, Matera J, Repollet M, Doyle GV, Terstappen LW, Hayes DF: Circulating tumor cells versus imaging–predicting overall survival in metastatic breast cancer. Clin Cancer Res. 2006, 12: 6403-6409. 10.1158/1078-0432.CCR-05-1769.
Allan AL, Keeney M: Circulating tumor cell analysis: technical and statistical onsiderations for application to the clinic. J Oncol. 2010, 2010: 426218-
Adams AA, Okagbare PI, Feng J, Hupert ML, Patterson D, Göttert J, McCarley RL, Nikitopoulos D, Murphy MC, Soper SA: Highly efficient circulating tumor cell isolation from whole blood and label-free enumeration using polymer-based microfluidics with an integrated conductivity sensor. J Am Chem Soc. 2008, 130: 8633-8641. 10.1021/ja8015022.
Kirby BJ, Jodari M, Loftus MS, Gakhar G, Pratt ED, Chanel-Vos C, Gleghorn JP, Santana SM, Liu H, Smith JP, Navarro NV, Tagawa ST, Bander NH, Nanus DM, Giannakakou P: Functional characterization of circulating tumor cells with a prostate-cancer-specific microfluidic device. PLoS One. 2012, 7: e35976-10.1371/journal.pone.0035976. Epub 32012 Apr 35927
Dancey JE, Dobbin KK, Groshen S, Jessup JM, Hruszkewycz AH, Koehler M, Parchment R, Ratain MJ, Shankar LK, Stadler WM, True LD, Gravell A: Grever MR; Biomarkers Task Force of the NCI Investigational Drug Steering Committee: Guidelines for the development and incorporation of biomarker studies in early clinical trials of novel agents. Clin Cancer Res. 2010, 16: 1745-1755. 10.1158/1078-0432.CCR-09-2167.
Allard WJ, Matera J, Miller MC, Repollet M, Connelly MC, Rao C, Tibbe AG, Uhr JW, Terstappen LW: Tumor cells circulate in the peripheral blood of all major carcinomas but not in healthy subjects or patients with nonmalignant diseases. Clin Cancer Res. 2004, 10: 6897-6904. 10.1158/1078-0432.CCR-04-0378.
Meng S, Tripathy D, Frenkel EP, Shete S, Naftalis EZ, Huth JF, Beitsch PD, Leitch M, Hoover S, Euhus D, Haley B, Morrison L, Fleming TP, Herlyn D, Terstappen LW, Fehm T, Tucker TF, Lane N, Wang J, Uhr JW: Circulating tumor cells in patients with breast cancer dormancy. Clin Cancer Res. 2004, 10: 8152-8162. 10.1158/1078-0432.CCR-04-1110.
Smerage JB, Doyle GV, Budd GT, Schott AF, Blayney DW, Wicha MS, Repollet M, Terstappen LW, Hayes DF: The detection of apoptosis and Bcl-2 expression in circulating tumor cells (CTCs) from women being treated for metastatic breast cancer. Proc Am Assoc Cancer Res. 2006, 47: abstr 792-
Taube SE, Clark GM, Dancey JE, McShane LM, Sigman CC, Gutman SI: A perspective on challenges and issues in biomarker development and drug and biomarker codevelopment. J Natl Cancer Inst. 2009, 101: 1453-1463. 10.1093/jnci/djp334.
Lianidou ES: Circulating tumor cells--new challenges ahead. Clin Chem. 2012, 58: 805-807. 10.1373/clinchem.2011.180646.
Hayes DF, Smerage J: Is there a role for circulating tumor cells in the management of breast cancer?. Clin Cancer Res. 2008, 14: 3646-3650. 10.1158/1078-0432.CCR-07-4481.
Reyal F, Valet F, de Cremoux P, Mathiot C, Decraene C, Asselain B, Brain E, Delaloge S, Giacchetti S, Marty M, Pierga JY, Bidard FC: Circulating tumor cell detection and transcriptomic profiles in early breast cancer patients. Ann Oncol. 2011, 22: 1458-1459. 10.1093/annonc/mdr144.
The authors would like to acknowledge discussions with other members of the CSC, developers of new CTC assays, and attendees at the CTC Workshop in 2010 as contributions to this manuscript. The authors are grateful to the Biomarkers Consortium and especially its Director, David Wholley for support of the CTC project and to Dr. J. Milburn Jessup of NCI and Drs. Elizabeth Mansfield and Robert Becker of the FDA for review of this manuscript. The authors thank Barbara Gress for literature research and Lora Smith and Susan Thompson for editorial assistance in completing the manuscript.
1New Enterprise Associates, Menlo Park, CA 94025, USA. 2Johnson & Johnson, Radnor, PA 19087, USA. 3CCS Associates, Mountain View, CA 94043, USA.4Critical Path Institute, Tucson, AZ 85718, USA. 5Fox Chase Cancer Center, Philadelphia, PA 19111, USA. 6Center for Drug Evaluation Research, US Food & Drug Administration, Silver Spring, MA 20903, USA. 7University of Michigan, Ann Arbor, MI 48109, USA. 8Covance Genomic Lab, Covance Central Labs, Seattle, WA 98382, USA. 9Daiichi-Sankyo Pharma Development, Edison, NJ 08837, USA. 10National Cancer Institute, Bethesda, MA 20892, USA.11Georgetown University, Washington, DC 20007, USA. 12Veridex, LLC, Raritan, NJ 08869, USA. 13EMD Serono, Rockland, MA 02370, USA. 14University Medical Center Hamburg-Eppendorf, 20246, Hamburg, Germany.15Foundation for the National Institutes of Health, Bethesda, MA 20814, USA.16Genentech, South San Francisco, CA 94080, USA. 17GlaxoSmithKline, Collegeville, PA 19426, USA. 18Eli Lilly and Company, Indianapolis, IN 46285, USA. 19Memorial Sloan-Kettering Cancer Center, New York, NY 10065, USA.
Several of the authors are past or current employees of, stockholders in, consultants to, or have received research funding or honoraria from Veridex LLC, the manufacturer of the CellSearch System™ for detection of CTCs, or its parent company Johnson & Johnson (ND, DH, MCL, RM, KP, HS). DH has also been a consultant to Biomarker Strategies of Baltimore, Maryland on CTCs and is named as an inventor or co-inventor on patents on applying CTCs in clinical settings. MC is a consultant to Alere, Inc. on CTCs; GK is an employee and stockholder of Covance, Inc., which includes CTC assays (particularly the Veridex CellSearch™ system) among its commercial offerings; and DP has been an employee of Nodality, Inc. which is developing technology that has potential application in CTC analysis. The remaining authors have no relevant competing interests (CC, BGP, AD, GJK, PK, JL, SM, LN, SPW, EP, LR, AS, CCS).
All authors contributed to the scientific and technical material presented in the manuscript, either by providing information based on direct experience with CTC technologies or relevant experience in developing biomarkers for clinical use. DP, co-chair of the Biomarkers Consortium CSC and of the CWG, led overall development of the manuscript. GJK, co-chair of the Biomarkers Consortium CSC, ensured that aspects of CTC science relevant to development of CTCs as biomarkers for predictive and prognostic applications in oncologic development were incorporated in the manuscript. BGP and CCS were responsible for background research and drafting the manuscript. Note that the contributions of AD to this manuscript are from his perspective and do not necessarily represent the views of the FDA. All authors read and approved the final manuscript.
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Parkinson, D.R., Dracopoli, N., Petty, B.G. et al. Considerations in the development of circulating tumor cell technology for clinical use. J Transl Med 10, 138 (2012). https://doi.org/10.1186/1479-5876-10-138