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Oncotarget. 2016 November 29; 7(48): 78421–78432.
Published online 2016 May 15. doi:  10.18632/oncotarget.9382
PMCID: PMC5346650

A novel microfluidic model can mimic organ-specific metastasis of circulating tumor cells

Abstract

A biomimetic microsystem might compensate costly and time-consuming animal metastatic models. Herein we developed a biomimetic microfluidic model to study cancer metastasis. Primary cells isolated from different organs were cultured on the microlfuidic model to represent individual organs. Breast and salivary gland cancer cells were driven to flow over primary cell culture chambers, mimicking dynamic adhesion of circulating tumor cells (CTCs) to endothelium in vivo. These flowing artificial CTCs showed different metastatic potentials to lung on the microfluidic model. The traditional nude mouse model of lung metastasis was performed to investigate the physiological similarity of the microfluidic model to animal models. It was found that the metastatic potential of different cancer cells assessed by the microfluidic model was in agreement with that assessed by the nude mouse model. Furthermore, it was demonstrated that the metastatic inhibitor AMD3100 inhibited lung metastasis effectively in both the microfluidic model and the nude mouse model. Then the microfluidic model was used to mimick liver and bone metastasis of CTCs and confirm the potential for research of multiple-organ metastasis. Thus, the metastasis of CTCs to different organs was reconstituted on the microfluidic model. It may expand the capabilities of traditional cell culture models, providing a low-cost, time-saving, and rapid alternative to animal models.

Keywords: microfluidic, metastasis, circulating tumor cells, multi-organ, bionic model

INTRODUCTION

Metastasis represents a highly organized and organ-specific process, with multiple destinations such as the lung, liver, and bone [14]. There are multiple steps of hematogenous metastasis, including degradation of the extracellular matrix, intravasation into blood vessels, surviving in the circulation, and extravastion into distant organs. Individual cancer cells involved in this metastasis that detach from the original tumor and circulate through the blood stream are called circulating tumor cells (CTCs), and are considered responsible for the metastasis [5].

Experimental metastatic models not only improve our understanding of the mechanisms of metastasis, but also serve as a platform to screen anti-metastatic drugs. Animal models has been considered the standard method to study metastasis [68]. Generally, there are two ways to model organ specific metastasis of human cancers using laboratory mice. The first is orthotopic transplantation of human cancer cells into mice. Using this methodology, it may take several months to form histologically detectable metastasis [912]. Alternatively, cancer cells can be injected directly into the systemic circulation of animals to mimic CTCs and accelerate metastasis. Metastasis usually occurs after several weeks. Overall, CTC metastasis to multiple organs can be well reproduced by animal models. However, these models involve complicated procedures, and are expensive and time-consuming, resulting in the high cost of pharmaceuticals and delayed development of new drugs [7, 1318]. In contrast, most in vitro metastatic models involve simple procedures, and are inexpensive and time-saving, such as the widely-used Transwells®. However, by culturing cells in a static condition, these Transwells® are unable to accurately reproduce the dynamic adhesion of CTCs to endothelium [19, 20].

A biomimetic microsystem reproducing the dynamic CTC metastasis to multiple organs may offer a solution to overcome the disadvantages of animal models, while facilitating the simple, inexpensive, and time-saving advantages of the Transwell® system. As a new technology, microfluidics creates new opportunities for spatial and temporal control of cell growth and stimuli. Microfabricated devices have been developed to facilitate both applied and basic research concerning the biology of cells, tissues, even organs [2126]. It has been emerging as an ideal platform to construct biomimetic models. These integrated microsystems can replicate the complex physiological functions of living organs, such as the functional alveolar capillary interface of the human lung. Some mcrofluidic-based platforms have been developed to replicate cancer invasion and metastatic processes [2732]. However, currently there have been no reports that have described engineering of integrated microsystems that replicate the complex CTCs metastasis by incorporating multiple organs, microvessels, and CTCs, and then placing them in a dynamic microenvironment.

In the present study, we describe the development of a microfluidic model to mimic multiple organ metastasis of CTCs. Using this microfluidic model, we modeled the potential of breast and salivary gland cancer cells to metastasize to the lung. When compared with traditional nude mouse model, similar results to those obtained from the microfluidic model were revealed. It demonstrated that this biomimetic model facilitated the rapid study of lung metastasis of CTCs. When we used this biomimetic model to evaluate the ability of antimetastatic agents to inhibit lung metastasis of breast cancer cells, similar effects were observed for both the microfluidic model and nude mouse model. Furthermore, the microfluidic model was used to mimick liver and bone metastasis of CTCs and confirmed the potential for research of multiple-organ metastasis.

RESULTS

Reconstitution of the microfluidic multiple organ model

The microfluidic model was composed of four layers: one layer of glass substrate, two layers of a PDMS (polydimethylsiloxane) membrane, and one layer of a porous polycarbonate membrane with 3 μm pore size and 6 μm thickness (Figure (Figure1A).1A). PDMS is widely used in microfluidic platforms for biological research because of its good biocompatibility and gas permeability. The bottom PDMS layer contained four separate organ chambers. Each chamber had its own inlet and outlet. The top PDMS layer contained four parallel microchannels (60 μm height and 400 μm width) that joined together at the cell reservoir at one end and at the syringe pump connector at the other end. The four microchannels were located on the top of four organ chambers, respectively. A transparent polycarbonate membrane separated each chamber and microchannel. The established microfluidic model was shown in Figure Figure1B.1B. A syringe pump was connected to the microchannels to drive the flow of CTCs via the syringe pump connector.

Figure 1
Reconstitution of the microfluidic model

In order to mimic the endothelial barrier of blood vessels, human umbilical vein endothelial cells (HUVEC) were seeded in the microchannels, pre-coated with Cultrex Basement Membrane Extracts (BME), a substitution of extracellular matrix, via the cell reservoir at first. Primary cells were loaded into the organ chambers via individual inlets. HUVEC cells attached to the porous membrane and formed a monolayer barrier, to mimic the barrier in vivo (Figure (Figure2A).2A). ZO-1 expression was confirmed, indicating the tight junction of HUVEC cells (Figure (Figure2B).2B). To characterize the permeability of the HUVEC barrier, fluorescein isothiocyanate-dextran (10 kDa) was introduced into each organ chamber. The fluorescein diffused from the chamber into the microchannels with time (Figure (Figure2C).2C). Quantitative analysis demonstrated that the fluorescence intensity increased with time, reached a steady state after 20 minutes, and remained stable during the time of the experiment (Figure (Figure2D2D).

Figure 2
Mimicking the vascular endothelial barrier on the microfluidic

Chemokine-induced metastasis in the microfluidic model

Chemokine CXCL12 is involved in metastasis via bonding to CXCR4, which is expressed on cell membranes in a wide variety of tumors [33, 34]. Furthermore, flow cytometry and immunofluorescent staining with anti-CXCR4 antibody indicated that MCF7, MDA-MB-231, and ACC-M cells expressed CXCR4 (Figure (Figure3A).3A). We therefore determined CXCL12-induced metastasis of MCF7, MDA-MB-231, and ACC-M cells using the microfluidic model. It was found that some of the flowing tumor cells stopped and attached to HUVEC cells when they passed over the top of the organ chambers containing CXCL12. The number of attached tumor cells gradually increased with CXCL12 concentration (Figure (Figure3B3B and and3C).3C). Furthermore, the arrested MDA-MB-231 cells significantly increased with 50 ng/mL and 100 ng/mL of CXCL12, while the arrested ACC-M cells significantly increased only with 100 ng/mL CXCL12. In contrast, the arrested MCF7 cells increased with a high concentration of CXCL12, but not in a significant manner.

Figure 3
Chemokine-induced metastasis of CTCs in the microfluidic model

Lung metastasis in microfluidic model

Lung metastatic model is widely used in the study of both breast and salivary gland cancers [35, 36]. The capabilities of lung metastasis of MCF7, MAD-MB-231, and ACC-M cells were assessed in the microfluidic model. Mixed primary cells isolated from the lung of SD rat were used to represent the lung. Primary muscle cells were used as a control. These primary cells showed good viability (Figure (Figure4A).4A). Quantitative analysis of CXCL12 expression by ELISA showed that CXCL12 was expressed in primary lung cells, but showed markedly low expression in primary muscle cells (Figure (Figure4A).4A). The primary cells were seeded into the organ chambers of the microfluidic model, respectively. When MCF7, MDA-MB-231, and ACC-M cells flowed over the cell organ chambers, different numbers of tumor cells stopped and attached to HUVEC (Figure (Figure4B).4B). Statistical analysis showed that the numbers of arrested MCF7, MDA-MB-231, and ACC-M cells by lung cells were significantly higher than those arrested by muscle cells (Figure (Figure4C).4C). In addition, MDA-MB-231 cells showed the strongest lung metastatic capability among the three cancer cell lines tested in the microfluidic model (Figure (Figure4D4D).

Figure 4
Lung metastasis in microfluidic model

Physiological similarity of the biomimetic microfluidic model to animal models

To further investigate the physiological similarity of the microfluidic model to animal models, we performed lung metastatic assays using the traditional nude mouse model and compared the metastatic capabilities of MCF7, MDA-MB-231, and ACC-M cells using the microfluidic and animal models. Fifteen nude mice were equally divided into three groups, and MCF7, MDA-MB-231, and ACC-M cells were inoculated into the tail vein. After one month, lung metastasis of each mouse was histologically examined. As shown in Figure 5A–5C, metastatic colonies of various sizes formed in lung. Consistent with MCF7 cells showing the lowest metastatic capability using the microfluidic model, the metastasis rates of MCF7, MDA-MB-231, and ACC-M were 80%, 100% and 100%, respectively. The colony numbers of MDA-MB-231 and ACC-M were also higher than that of MCF7, but not significantly (Figure (Figure5D).5D). We compared the colony areas per lung of MCF7, MDA-MB-231, and ACC-M cells. It was found that MDA-MB-231 showed the highest metastatic capability among the three cancer cell lines (p < 0.05) (Figure (Figure5E),5E), which was consistent with that assessed by the microfluidic model (Figure (Figure4D4D).

Figure 5
Physiological similarity of the microfluidic model to the animal model

Inhibition of lung metastasis in the microfluidic model and mouse model

The microfluidic model was then used to evaluate the inhibitory effect of anti-metastatic drugs. AMD3100, a small molecule antagonist of CXCR4, has been reported to inhibit CXCL12-induced tumor metastasis [37, 38]. When AMD3100 was tested using the microfluidic model with primary lung cells in organ chambers, the number of cancer cells attached to the HUVEC layer was reduced gradually by increasing the AMD3100 concentration (Figure (Figure6A).6A). These results suggest that AMD3100 significantly inhibited lung metastasis of MDA-MB-231 cells (p < 0.05). Nude mice were then treated with AMD3100, and the results of this in vivo model compared with the results obtained from the microfluidic model. In a similar manner as the microfluidic model, the colony areas significantly decreased with AMD3100 treatment (p < 0.05) (Figure (Figure6B).6B). This suggests that AMD3100 inhibited lung metastasis of MDA-MB-231 cells in nude mice, as assessed both by metastatic areas and colonies per lung section.

Figure 6
Inhibition of lung metastasis in the microfluidic model and nude mouse model

Liver and bone metastasis in the microfluidic model

In addition to the lung, liver and bone marrow are common metastatic sites in both breast and salivary gland cancers [35, 36]. To demonstrate the potential of assessing multi-organ metastasis in the microfluidic model, primary cells isolated from liver and bone marrow were used to represent specific organs. Primary muscle cells were used as a control. These primary cells showed good viability of over 90% (Figure (Figure7A).7A). Quantitative analysis of CXCL12 expression by ELISA showed that CXCL12 was expressed in primary liver and bone marrow cells, but showed markedly low expression in primary muscle cells (Figure (Figure7A).7A). The three types of primary cells were seeded into the organ chambers of the microfluidic model, respectively, so that each chamber represented a specific organ. When MCF7, MDA-MB-231, and ACC-M cells flowed over the cell organ chambers, different numbers of tumor cells stopped and attached to HUVEC (Figure (Figure7B).7B). Statistical analysis showed that the numbers of arrested MCF7, MDA-MB-231, and ACC-M cells by liver, and bone marrow cells were significantly higher than those arrested by muscle cells (p < 0.01) (Figure (Figure7C7C).

Figure 7
Liver and bone metastasis of CTCs in the microfluidic model

DISCUSSION

Biomimetic models that can reproduce complex and integrated physiological and pathological events are important alternatives to animal models in basic biological research and drug development. In the present study, we developed a microfluidic model that reproduced the organ-specific metastasis of CTCs (Figure (Figure8).8). To reconstitute multiple organs on the microfluidic model, primary cells of mouse organs were isolated and cultured in organ chambers. These primary cells retained many characteristics of the original organs, such as secreting different levels of chemokines using the microfluidic model. Chemokines approximately 10,000 Da in size could diffuse from organ chambers into microchannels, to act as attractants of CTCs to facilitate the metastatic process.

Figure 8
llustration of organ-specific metastasis of CTCs in the microfluidic chip

Adhesion between flowing CTCs and the microvascular endothelium of specific organs is a key step in hematogenous metastasis [39, 40]. Shear stress generated by the flow can inhibit the adhesion between CTCs and endothelium to further decrease metastasis [41, 42]. To reproduce the in vivo flowing condition of CTCs, a physiological flow rate was used in the microfluidic model. Overall, multiple organs, microvessels with endothelium, and flowing CTCs were integrated in the microfluidic model, and the metastatic potentials of MCF7, MDA-MB-231, and ACC-M cells toward multiple organs could be assessed. The three tumor cell lines tested showed significantly higher metastatic potentials to lung, liver, and bone marrow cells than to muscle cells. This result was consistent with clinical observations. Together, the results demonstrated that the bimimetic multiple organ model provided a novel platform for the study of organ-specific metastasis of CTCs.

We wanted to determine if our microfluidic model had the physiological similarity to traditional metastatic animal models such as the nude mouse. Lung is the most common metastatic destination in many cancers. To establish the lung mestatasis animal model, tumor cells are injected into the mouse tail vein. Usally, it takes over 3 weeks to form detectable metastases as assessed by histological examination. We compared the metastatic capabilities of MCF7, MDA-MB-231, and ACC-M cells assessed by the microfluidic model with this traditional lung metastasis animal model. It was found that the results obtained by the microfluidic model were consistent with results obtained from the animal model. This result strongly suggested, at least for lung metastasis, that the microfluidic model had the potential to mimick the animal model. Furthermore, compared to the animal model, the microfluidic model was simpler to operate, less expensive, and significantly more time-saving, taking only 2 days to perform metastatic tests.

To investigate whether this microfluidic model could be used to rapidly and inexpensively screen drugs for their potential to inhibit metastasis, the ability of AMD3100 to inhibit MDA-MB-231 metastasis was directly compared using the microfluidic and animal models. AMD3100, also named Plerixafor, is an antagonist of CXCR4 which is clinically used to treat non-Hodgkin's lymphoma and multiple myeloma [43]. The results with both the microfluidic and animal models showed that AMD3100 was able to reduce the lung metastasis of MDA-MB-231. Because the adhesion of CTCs to endothelium were reproduced in the microfluidic model, agents targeting CTC adhesion can now be rapidly screened using this model. And the microfluidic model can be used in preclinical tests to assess the abilities of new compounds to inhibit several processes in organ-specific metastasis.

Regarding limitations of the present study, we only used the microfluidic model and animal models to compare the capability of cancer cells to metastasize to the lung. In animal models, metastasis is largely influenced by both the site of injection and the metastatic capacity of tumor cells. Injection routes include the lateral tail vein, plus other intraportal, intracarotid, and intracardiac sites. Tail vein injection is the most commonly used assay, and primarily leads to lung metastasis. Intraportal vein injection usually results in liver metastasis, while intracarotid injection leads to brain metastasis. Only intracardiac injection can result in metastasis to multiple organs (such as bone, liver, brain, and lung) because tumor cells are introduced into the arterial circulation. However, intracardiac injection is a difficult procedure and has a very high mortality rate, because injected tumor cells can induce a hypercoagulable state that leads to platelet consumption and thromboemboli formation [44]. Nonetheless, future studies should be conducted to compare the microfluidic model with other animal models of metastasis.

MATERIALS AND METHODS

Ethical statement

Animal experiments, transportation, and care were conducted in compliance with the relevant laws and the guidelines issued by the Ethical Committee of Dalian Medical University. The experimental groups had five mice per group and the control group had five mice. Animals were fed in the SPF level laboratory. They were sacrificed after 30 days.

Additional methods

Additional methods involving fabrication of the microfluidic device, culture and labeling of cells, immunofluorescent staining, isolation of primary mouse cells, assessment of cell viability, and determination of CXCL12 secretion from primary cells can be found in the Supplementary Methods.

Chemokine-induced metastasis assay using the microfluidic model

HUVECs have been previously reported to be served as the vascular endothelial barrier [29, 31, 45, 46]. Similarly, they were seeded onto the porous membrane of the device, which was pre-coated with BME (R&D Systems, Minneapolis, MN, USA), and cultured for 24 hours to mimic vascular endothelial barrier. CXCL12 as the member of chemokine family play an important role of metastasis. Different concentrations (0 ng/mL, 25 ng/mL, 50 ng/mL, and 100 ng/mL) of recombinant CXCL12 (R&D Systems) were loaded into each organ chamber and incubated for 5 hours. Tumor cells were cultured with serum-free medium for 5 hours, then harvested and loaded into the cell reservoir at a concentration of 2 × 106 cells/mL. Then a syringe pump (Baoding Longer Precision Pump Co., Ltd, Baoding, China) was connected. The flow rate (750 nL/minute) was adjusted to almost the same as that of microvessels in vivo. Driven by the syringe pump, tumor cells flowed into the microchannels at a constant rate for 20 minutes, then the cells were incubated for another 10 minutes after stopping the pump. Phosphate-buffered saline (PBS) was used to remove loosely attached cells. At least three images were recorded randomly for each microchannel at 100× magnification using an inverted fluorescent microscope (Olympus IX71, Olympus Corp., Tokyo, Japan). Image-Pro® Plus version 6.0 (Media Cybernetics, Inc. Silver Spring, MD, USA) software was used to count the number of tumor cells arrested on HUVEC cells in the microchannels. Each experiment was repeated at least eight times.

Organ-specific metastasis assay using the microfluidic device

The organ chambers of the device were coated with collagen I (Life Technologies Corp., Gaithersburg, MD, USA) before cell seeding. Mixed primary cells isolated from specific organs of SD rats were then seeded into individual organ chambers. The total numbers of mixed primary cells are 4 × 105 cells in individual organ chambers. HUVEC cells were seeded on the porous membrane, then the device was incubated at 37°C in 5% CO2 for 24 hours. Tumor cells were loaded into the cell reservoir at a concentration of 2 × 106 cells/mL, and a syringe pump was connected with the syringe pump connector to drive the flow of tumor cells. The same assay steps were used to measure chemokine-induced metastasis.

In vivo metastasis assay using a nude mouse model

BALB/c nude mice aged 4−5 weeks old (18 g, female, Dalian Medical University Laboratory Animal Center) were used to assess the in vivo metastatic capability of tumor cells. Mice were divided into three groups according to type of transplanted tumor cells: the MCF7 group, the MDA-MB-231 group, and the ACC-M group, with five mice in each group. Cells were harvested and resuspended at a concentration of 2 × 106 cells/mL in PBS, then injected into the tail vein. The nude mice were raised in sterile conditions for 30 days, then euthanized and the lung tissues removed. Tissues were fixed in 10% formalin for 24 hours and embedded in paraffin. Sections of 4 μm thickness were prepared and stained with hematoxylin and eosin (H.E.). Immunohistochamical staining with anti-humna Pan CK (Merckmillipore, USA) was performed to detect the metastatic colonies. The images were recorded by a microscope (Olympus BX43, Olympus Corp., Tokyo, Japan). The images were recorded by a microscope (Olympus BX43, Olympus Corp., Tokyo, Japan). Metastatic rate and metastatic colony areas per lung section were used to evaluate the metastatic capability of each tumor cell line. Metastasis was regarded as positive even if only one metastatic colony was found in the lung. Metastatic rate was represented as the ratio of animals with positive metastasis in all experimental animals. High power view images (400×) were used to calculate metastatic colony areas. Firstly, the colonies were confirmed by H.E. and anti-human Pan cytokeratin immunostaining and circumscribed using Image-Pro® Plus version 6.0 software. The metastatic areas were determined as the total areas of all metastatic colonies in the lung.

Inhibition of lung metastasis by AMD3100 using the microfluidic device and mouse models

To inhibit lung metastasis in vitro, the anti-metastatic reagent AMD3100 (Sigma, St. Louis, MO, USA) was used. Different concentrations of AMD3100 (0 μg/mL, 0.5 μg/mL, 1 μg/mL, and 2 μg/mL) were introduced into the microchannels and incubated overnight. Tumor cells were resuspended at a concentration of 2 × 106 cells/mL in culture medium with AMD3100 and loaded into the cell reservoir, followed by the same assay steps as previously described.

To inhibit lung metastasis in vivo, AMD3100 (Sigma) was used in a mouse model. Three hours after injection of tumor cells into the tail vein, five BALB/c-nude mice (4−5 weeks old, female) were subcutaneously treated with 1.25 mg/kg AMD3100, followed by AMD3100 treatment twice daily. After 30 days, the mice were euthanized, and lung tissues were dissected and submitted for histological examination.

Statistical analysis

Statistical analyses were performed using SPSS version 13.0 for Windows (SPSS Inc., Chicago, IL, USA). The independent sample nonparametric-test was used to analyze comparisons of all data and were expressed as mean ± SE. Each experiment was conducted at least three times, and significance was identified as a p value of < 0.05.

CONCLUSIONS

In summary, we have developed a microfluidic multiple organ model to reproduce organ specific metastasis of CTCs. Comparisons between this microfluidic model and the nude mouse model demonstrated that the microfluidic model has the similarity to the metastatic animal model. Overall, this multiple organ model shows a certain potential to provide an inexpensive and time-saving alternative to animal models, to predict the metastatic capabilities of different CTCs for specific organs, and to rapidly screen possible anti-metastatic drugs.

SUPPLEMENTARY MATERIALS

ACKNOWLEDGMENTS AND FUNDING

This work was supported by National Natural Science Foundation of China (No.81171425) and National Major Scientific and Technological Special Project for “Significant New Drugs Development” (2013ZX09507005).

Footnotes

CONFLICTS OF INTEREST

There has no conflicts of interest declaration.

REFERENCES

1. Fidler IJ. The pathogenesis of cancer metastasis: the'seed and soil'hypothesis revisited. Nat Rev Cancer. 2003;3:453–458. [PubMed]
2. Nguyen DX, Bos PD, Massagué J. Metastasis: from dissemination to organ-specific colonization. Nat Rev Cancer. 2009;9:274–284. [PubMed]
3. Billingsley KG, Burt ME, Jara E, Ginsberg RJ, Woodruff JM, Leung DH, Brennan MF. Pulmonary metastases from soft tissue sarcoma: analysis of patterns of disease and postmetastasis survival. Ann Surg. 1999;229:602. [PubMed]
4. Hess KR, Varadhachary GR, Taylor SH, Wei W, Raber MN, Lenzi R, Abbruzzese JL. Metastatic patterns in adenocarcinoma. Cancer. 2006;106:1624–1633. [PubMed]
5. Cristofanilli M, Budd GT, Ellis MJ, Stopeck A, Matera J, Miller MC, Reuben JM, Doyle GV, Allard WJ, Terstappen LW. Circulating tumor cells, disease progression, and survival in metastatic breast cancer. N Engl J Med. 2004;351:781–791. [PubMed]
6. Frese KK, Tuveson DA. Maximizing mouse cancer models. Nat Rev Cancer. 2007;7:654–658. [PubMed]
7. Khanna C, Hunter K. Modeling metastasis in vivo. Carcinogenesis. 2005;26:513–523. [PubMed]
8. Zhu G, Yan H, Pang Y, Jian J, Achyut B, Liang X, Weiss J, Wiltrout R, Hollander M, Yang L. CXCR3 as a molecular target in breast cancer metastasis: inhibition of tumor cell migration and promotion of host anti-tumor immunity. Oncotarget. 2015;6:43408–43419. doi: 10.18632/oncotarget.6125. [PMC free article] [PubMed] [Cross Ref]
9. Hoffman RM. Orthotopic metastatic mouse models for anticancer drug discovery and evaluation: a bridge to the clinic. Invest New Drugs. 1999;17:343–360. [PubMed]
10. Kubota T. Metastatic models of human cancer xenografted in the nude mouse: the importance of orthotopic transplantation. J Cell Biochem. 1994;56:4–8. [PubMed]
11. Iorns E, Drews-Elger K, Ward TM, Dean S, Clarke J, Berry D, El Ashry D, Lippman M. A new mouse model for the study of human breast cancer metastasis. PloS one. 2012;7:e47995. [PMC free article] [PubMed]
12. Céspedes MV, Casanova I, Parreño M, Mangues R. Mouse models in oncogenesis and cancer therapy. Clin Transl Oncol. 2006;8:318–329. [PubMed]
13. Minn AJ, Gupta GP, Siegel PM, Bos PD, Shu W, Giri DD, Viale A, Olshen AB, Gerald WL, Massagué J. Genes that mediate breast cancer metastasis to lung. Nature. 2005;436:518–524. [PMC free article] [PubMed]
14. Lim C, Cauchy F, Azoulay D, Farges O, Ronot M, Pocard M. Tumour progression and liver regeneration—insights from animal models. Nat Rev Gastro Hepat. 2013;10:452–462. [PubMed]
15. Lorger M, Felding-Habermann B. Capturing changes in the brain microenvironment during initial steps of breast cancer brain metastasis. Am J Pathol. 2010;176:2958–2971. [PubMed]
16. Arguello F, Baggs RB, Frantz CN. A murine model of experimental metastasis to bone and bone marrow. Cancer Res. 1988;48:6876–6881. [PubMed]
17. Jenkins DE, Hornig YS, Oei Y, Dusich J, Purchio T. Bioluminescent human breast cancer cell lines that permit rapid and sensitive in vivo detection of mammary tumors and multiple metastases in immune deficient mice. Breast Cancer Res. 2005;7:R444–R454. [PMC free article] [PubMed]
18. Prensner JR, Iyer MK, Sahu A, Asangani IA, Cao Q, Patel L, Vergara IA, Davicioni E, Erho N, Ghadessi M. The long noncoding RNA SChLAP1 promotes aggressive prostate cancer and antagonizes the SWI/SNF complex. Nat Genet. 2013 [PMC free article] [PubMed]
19. Hooper S, Marshall JF, Sahai E. Tumor cell migration in three dimensions. Methods Enzymol. 2006;406:625–643. [PubMed]
20. Zimmermann M, Box C, Eccles SA. Two-dimensional vs. three-dimensional in vitro tumor migration and invasion assays. Target Identification and Validation in Drug Discovery. (Springer) 2013:227–252. [PubMed]
21. Huh D, Hamilton GA, Ingber DE. From 3D cell culture to organs-on-chips. Trends Cell Biol. 2011;21:745–754. [PMC free article] [PubMed]
22. Kim S, Lee H, Chung M, Jeon NL. Engineering of functional, perfusable 3D microvascular networks on a chip. Lab Chip. 2013;13:1489–1500. [PubMed]
23. Huh D, Matthews BD, Mammoto A, Montoya-Zavala M, Hsin HY, Ingber DE. Reconstituting organ-level lung functions on a chip. Science. 2010;328:1662–1668. [PubMed]
24. Lee PJ, Hung PJ, Lee LP. An artificial liver sinusoid with a microfluidic endothelial-like barrier for primary hepatocyte culture. Biotechnol Bioeng. 2007;97:1340–1346. [PubMed]
25. Imura Y, Asano Y, Sato K, Yoshimura E. A microfluidic system to evaluate intestinal absorption. Anal Sci. 2009;25:1403–1407. [PubMed]
26. Jang K-J, Suh K-Y. A multi-layer microfluidic device for efficient culture and analysis of renal tubular cells. Lab Chip. 2010;10:36–42. [PubMed]
27. Albanese A, Lam AK, Sykes EA, Rocheleau JV, Chan WC. Tumour-on-a-chip provides an optical window into nanoparticle tissue transport. Nat commun. 2013:4. [PMC free article] [PubMed]
28. Zhang Q, Liu T, Qin J. A microfluidic-based device for study of transendothelial invasion of tumor aggregates in realtime. Lab chip. 2012;12:2837–2842. [PubMed]
29. Zervantonakis IK, Hughes-Alford SK, Charest JL, Condeelis JS, Gertler FB, Kamm RD. Three-dimensional microfluidic model for tumor cell intravasation and endothelial barrier function. Proc Natl Acad Sci USA. 2012;109:13515–13520. [PubMed]
30. Shin MK, Kim SK, Jung H. Integration of intra-and extravasation in one cell-based microfluidic chip for the study of cancer metastasis. Lab Chip. 2011;11:3880–3887. [PubMed]
31. Song JW, Cavnar SP, Walker AC, Luker KE, Gupta M, Tung Y-C, Luker GD, Takayama S. Microfluidic endothelium for studying the intravascular adhesion of metastatic breast cancer cells. PloS one. 2009;4:e5756. [PMC free article] [PubMed]
32. Li E, Xu Z, Zhao H, Sun Z, Wang L, Guo Z, Zhao Y, Gao Z, Wang Q. Macrophages promote benzopyrene-induced tumor transformation of human bronchial epithelial cells by activation of NF-κB and STAT3 signaling in a bionic airway chip culture and in animal models. Oncotarget. 2015;6:8900–8913. doi: 10.18632/oncotarget.3561. [PMC free article] [PubMed] [Cross Ref]
33. Domanska UM, Kruizinga RC, Nagengast WB, Timmer-Bosscha H, Huls G, de Vries EG, Walenkamp AM. A review on CXCR4/CXCL12 axis in oncology: no place to hide. Eur J Cancer. 2013;49:219–230. [PubMed]
34. Teicher BA, Fricker SP. CXCL12 (SDF-1)/CXCR4 pathway in cancer. Clin Cancer Res. 2010;16:2927–2931. [PubMed]
35. Müller A, Homey B, Soto H, Ge N, Catron D, Buchanan ME, McClanahan T, Murphy E, Yuan W, Wagner SN. Involvement of chemokine receptors in breast cancer metastasis. Nature. 2001;410:50–56. [PubMed]
36. van der Wal JE, Becking AG, Snow GB, van der Waal I. Distant metastases of adenoid cystic carcinoma of the salivary glands and the value of diagnostic examinations during follow-up. Head Neck. 2002;24:779–783. [PubMed]
37. Davies S, Serradell N, Bolos J, Bayes M. Plerixafor hydrochloride. Drug Today. 2007;32:123–136.
38. Smith MC, Luker KE, Garbow JR, Prior JL, Jackson E, Piwnica-Worms D, Luker GD. CXCR4 regulates growth of both primary and metastatic breast cancer. Cancer Res. 2004;64:8604–8612. [PubMed]
39. Pilch J, Habermann R, Felding-Habermann B. Unique ability of integrin αvβ3 to support tumor cell arrest under dynamic flow conditions. J Biol Chem. 2002;277:21930–21938. [PubMed]
40. Steeg PS. Tumor metastasis: mechanistic insights and clinical challenges. Nat Med. 2006;12:895–904. [PubMed]
41. Haier J, Nicolson GL. Tumor cell adhesion under hydrodynamic conditions of fluid flow. Apmis. 2001;109:241–262. [PubMed]
42. Lee A, Berny-Lang M, Liao S, Kanso E, Kuhn P, McCarty O, Newton P. A low-dimensional deformation model for cancer cells in flow. Phys Fluids. 2012;24:081903. [PubMed]
43. DiPersio JF, Stadtmauer EA, Nademanee A, Micallef IN, Stiff PJ, Kaufman JL, Maziarz RT, Hosing C, Früehauf S, Horwitz M. Plerixafor and G-CSF versus placebo and G-CSF to mobilize hematopoietic stem cells for autologous stem cell transplantation in patients with multiple myeloma. Blood. 2009;113:5720–5726. [PubMed]
44. Schuh JC. Trials, tribulations, and trends in tumor modeling in mice. Toxicol Pathol. 2004;32:53–66. [PubMed]
45. Buchanan CF, Verbridge SS, Vlachos PP, Rylander MN. Flow shear stress regulates endothelial barrier function and expression of angiogenic factors in a 3D microfluidic tumor vascular model. Cell Adhes Migr. 2014;8:517–524. [PMC free article] [PubMed]
46. Abaci HE, Shen Y-I, Tan S, Gerecht S. Recapitulating physiological and pathological shear stress and oxygen to model vasculature in health and disease. Sci Rep. 2014:4. [PMC free article] [PubMed]

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