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Gamma irradiation exposure for collapsed cell junctions and reduced angiogenesis of 3-D in vitro blood vessels

Abstract

During radiotherapy, microenvironments neighboring the tumor are also exposed to gamma irradiation; this results in unexpected side effects. Blood vessels can serve as microenvironments for tumors and they play an important role in providing nutrients to tumors. This is mostly related to tumor progression, metastasis, and relapse after therapy. Many studies have been performed to obtain a better understanding of tumor vasculature after radiotherapy with in vitro models. However, compared to 3-D models, 2-D in vitro endothelial monolayers cannot physiologically reflect in vivo blood vessels. We previously remodeled the extracellular matrix (ECM) hydrogel that enhanced the tight barrier formation of 3-D blood vessels and the vascular endothelial growth factor (VEGF) gradient induced angiogenesis in a microfluidic device. In this study, the blood vessel model is further introduced to understand how gamma irradiation affects the endothelial monolayer. After the gamma irradiation exposure, we observed a collapsed endothelial barrier and a reduced angiogenic potential. Changes in the cell behaviors of the tip and stalk cells were also detected in the angiogenesis model after irradiation, which is difficult to observe in 2-D monolayer models. Therefore, the 3-D in vitro blood vessel model can be used to understand radiation-induced endothelial injuries.

Introduction

Radiation treatment, which is also known as radiotherapy, has been widely applied to a variety of solid tumors in which it is used to kill the tumor cells directly or reduce the tumor mass1,2,3,4. There are several supportive cells in the tumor microenvironment and they can be damaged by radiation exposure, which can result in several side effects5,6,7,8. Blood vessels play an important role in supplying nutrients and oxygen to tumors; they also act as routes for other organs, which causes tumors to grow or become metastasized9,10,11,12,13. Indeed, as the tumor size increases, its metabolism is restricted owing to the limited diffusion of oxygen and nutrients. The tumor then recruits new blood vessels by secreting angiogenic activators such as vascular endothelial growth factor (VEGF), basic fibroblast growth factor (bFGF), and tumor necrosis factor alpha (TNF-a)14,15,16,17,18. Because these new blood vessels can affect the efficacy of in vivo radiotherapy for tumors, several kinds of anti-angiogenic drugs have been combined to suppress tumor regression effectively19,20.

Many researchers have reported that endothelial cells undergo changes in their molecular pathways and cell phenotypes after they are exposed to gamma irradiation21,22,23,24. In particular, the reorganization and reduction of cell–cell junctions between endothelial cells are major problems because they increase cell permeability and weaken barrier functions25,26,27. However, most of these studies were conducted on 2-D in vitro culture systems, in which the endothelial cells grow as a homogenous monolayer. As a result, they cannot reflect the physiological relevance of in vivo blood vessels. For instance, the morphology and biochemical signaling of the endothelial cells differ according to the cell–cell and cell–matrix interactions. In addition, soluble gradients such as nutrients, oxygen, and other stimuli are absent in 2-D culture systems28,29,30. Conversely, 3-D endothelial models have the potential to constitute more realistic biochemical and biomechanical microenvironments for blood vessels. These models can support diverse endothelial cell behaviors such as angiogenesis, vasculogenesis, and cell invasion.

In our previous research, we enhanced the permeability and barrier maintenance of a 3-D endothelial monolayer by remodeling the extracellular matrix (ECM) hydrogel. In addition, angiogenesis can be triggered by the VEGF gradient31,32. Because the majority of defects in irradiated endothelial cells result in a loss of barrier functions and cell motility, our 3-D endothelial cell model can be a powerful tool to understand the radiation damage to human blood vessels. This study demonstrates that gamma irradiation exposure weakens the barriers of the endothelial cell and it can be visualized through the diffusion of dextran molecules across the endothelial barriers. Furthermore, the genes that regulate the notch signaling pathway in angiogenesis, as well as the cell behaviors of the tip and stalk cells, change depending on the gamma irradiation doses. To the best of our knowledge, this is the first study to show how gamma irradiation exposure affects endothelial cell behaviors in the 3-D hydrogel-incorporated blood barrier model.

Materials and methods

Preparation of the microfluidic chip

The microfluidic channels were patterned by photolithography. First, the SU-8-100 photoresist (MicroChem, USA) was spin-coated onto a silicon wafer and then baked at 95 °C for 1 h. Using selective ultraviolet (UV) exposure, microfluidic channels were patterned on a silicon wafer. Polydimethylsiloxane (PDMS, SYLGARD 184, Dow, USA) was cured on this micropatterned silicon wafer with a conventional soft lithography procedure. Reservoirs were punched with 4 mm and 1 mm biopsy punches. The microfluidic chip was sterilized twice at 120 °C for 15 min and then dried at 80 °C overnight. The dried microfluidic chip and cover glass were bonded with an oxygen plasma treatment (FEMTOSCIENCE, Korea) for 1 min at 100 W. After the plasma treatment, the hydrophilic microchannels were filled with 1 mg/mL of PDL (poly-d-lysine, Sigma-Aldrich) hydrobromide solution to enhance the adhesion of the hydrogel to the surface of the PDMS and the cover glass. After incubating at 37 °C for 3 h, the microfluidic channels were washed twice with deionized distilled water (DW). The microfluidic chip was dried overnight at 80 °C and stored at room temperature before usage.

Cell preparation

Primary human dermal microvascular endothelial cells (hMVEC; Lonza, cat. no. CC2546, Switzerland) were purchased and cultured in an EGM-2MV bullet kit (Lonza, cat. no. CC3202, Switzerland) at 37 °C in a humidified 5% CO2 incubator. The hMVECs were maintained until ~ 70% confluence in a 75T flask. In this study, the hMVECs in passage six were used for the experiments.

ECM remodeling and cell seeding

Before seeding the cells, a pre-polymerized type I collagen (COL1) solution at a concentration of 2.0 mg/ml was prepared by dilution in a mixture of 10X phosphate buffered saline (PBS) and DW. In addition, the pH of the COL1 solution was adjusted with a 1.0 N NaOH solution. The COL1 solution was then poured into the four regions of the microfluidic chip. After pouring the COL1 solution, the chip was incubated at 37 °C for 30 min in a humidified chamber to prevent the hydrogel from drying. Subsequently, all the channels, except for the ECM channels, were filled with a cell culture medium, EGM-2MV. In a previously published paper from our laboratory, we showed that remodeling the ECM hydrogel results in a tight endothelial barrier in the microfluidic chip. Briefly, after the COL1 solution was poured into the gel regions and gelled, the cell culture channels were filled with serum-free culture medium. Then, growth factor reduced (GFR)-Matrigel solution (diluted in serum-free culture medium, 1:50) was added to the channels on ice for 5 min; this solution was coated onto the surface of the COL1 for more than 40 min in a 37 °C incubator. Subsequently, the hMVECs were harvested by trypsinization and seeded into the central channel of the microfluidic chip at a density of 2 × 104/cm2 after the culture medium was removed from the side channels. The hMVECs were attached to the ECM by hydrostatic pressure for 2 h in a 37 °C incubator. After being cultured in the microfluidic channel for 4 days, they formed a monolayer. The medium was exchanged every day.

Four days after cell seeding into the microfluidic chip, the hMVEC monolayers were exposed to gamma irradiation at 4 Gy and 8 Gy (BIOBEAM 8000, Gamma-Service Medical GmbH, Germany). After the gamma irradiation treatment, the hMVECs were cultured for more than 4 days. The medium was exchanged every day.

Permeability analysis

To measure the permeability of the endothelial cell monolayer in the microfluidic chip, 10 µM of 40 kDa fluorescein isothiocyanate (FITC)–dextran solution was added to the central hMVECs channel and incubated for 3 h at 37 °C. The value of the permeability was calculated using Fick’s first law:

\begin{aligned} & J = - D\frac{\partial C}{{\partial x}}, \\ & {\text{Flux}} = - P\Delta C, \\ \end{aligned}

where $$J$$ is the flux, $$D$$ is the diffusion coefficient, $$C$$ is the concentration, $$x$$ is the position, and $$P$$ is the permeability of the endothelial monolayer. The diffusion coefficient of 40 kDa FITC-dextran in ECM hydrogel was assumed as 43 µm2/s with reference33. And, the diffusion profile of FITC–dextran was captured by fluorescence imaging, and the distribution was analyzed with the ImageJ software program (7.0a, GraphPad, www.graphpad.com).

Immunofluorescence staining and quantification

The hMVECs in the microfluidic chip were fixed with 4% paraformaldehyde (PFA) at 25 °C for 30 min. Then, the cells were permeabilized with 0.1% Triton X-100 for 15 min at RT. In sequence, the cells were blocked with 3% bovine albumin serum (BSA) for 1 h at RT. Then, 50 µL of the diluted primary antibodies in the PBS solutions were added to the central channel and stored at 4 °C overnight. Secondary antibodies were conjugated with primary antibodies at RT for 1 h. All the primary and secondary antibodies are listed in Table 1. In each step, two sets of PBS washes were included. The fluorescence images were captured with a confocal laser-scanning microscope (LSM700; Carl Zeiss, Germany). Actin fibers were evaluated in total 45 randomly chosen hMVECs for each radiation doses and cells were divided into three groups differing in the number of actin stress fibers (0, 1–10, and > 10). The average intensity of VE-cadherin on cytoplasm and cell–cell border was measured by using Image J software program.

qRT-polymerase chain reaction (PCR) analysis

To extract the RNA from the hMVECs, the hMVECs in the microfluidic chip were harvested. Due to the number of hMVECs in one microfluidic chip was very small, hMVECs in about 5–10 microfluidic chips were collected as n number one (n = 2–3). Total RNA was isolated with the RNeasy Mini Kit (QIAGEN, Cat.no.74104, Germany) and the concentration of the total RNA was measured with a Nanodrop spectrophotometer (absorbance wavelength: 260 nm, ThermoFisher Scientific, Cat. no. ND-1000, USA). After the RNA normalization, cDNA was synthesized via reverse transcription with a high-capacity RNA-to-cDNA kit (Applied Biosystems, Cat.no. 4387406, USA) and StepOne Real-time PCR equipment (Applied Biosystems, Cat.no. Step-one plus, USA). We designed the PCR primers which are listed in Table 2. The PCR reactions were performed as duplicates using the StepOne system with the QuantiTect SYBR green PCR kit (QIAGEN, Cat.no. 204143, Germany). In addition, the gene expression of the target genes was normalized according to the housekeeping gene Gapdh and quantified with the comparative Ct method.

Inducing the migration of the hMVECs in a microfluidic chip after gamma irradiation

The migration and angiogenesis of the hMVECs were induced by VEGF. In our microfluidic chip, a chemical gradient can be generated and maintained between the central and side channels. To induce the migration of the hMVECs, we introduced additional VEGF-A (PeproTech, Cat.no. 100-20, USA) with 50 ng/mL to the side medium channels daily. Due to our goal is to investigate how the gamma irradiation affects angiogenesis, additional VEGF-A was supplied to the side channels for 5 days after radiation treatment.

Results

Endothelial barrier formation in a 3-D microfluidic chip

In our previous study, we fabricated a microfluidic chip for a 3-D cell culture that consisted of three parallel cell channels and four regions for hydrogel filling. In addition, we showed that Matrigel-coated type I collagen (BM-COL1) enhanced the barrier function of the endothelial cells with a high expression of tight and adhesion junctions31. In this study, we used this method to form a 3-D endothelial barrier, and hMVECs were used because this endothelial cell type displays superior barrier properties in comparison to umbilical vein endothelial cells (hUVECs)34. In our microfluidic chip, a hydrostatic pressure difference can be developed between the channels; this makes the cells more efficiently attached to BM-COL1. In addition, we determined that the hMVECs in the central channel proliferated and formed a confluent monolayer within 4 days after seeding the cells (Fig. 1a). To investigate how the gamma irradiation exposure affects the endothelial barrier, we exposed the monolayer of the hMVECs in the microfluidic chip to three doses (0 Gy for the control, 4 Gy, and 8 Gy) of gamma irradiation (Fig. 1b).

Changes in the actin filament structures when subjected to gamma irradiation

The actin filaments, which are also known as F-actin, are polymeric filaments that are composed of many globular actins (G-actins). They can determine the cell morphology and motility by actin polymerization. Likewise, these actin filaments in endothelial cells are important for controlling several kinds of cellular processes, which include cell–cell adhesion and cell migration35,36,37. Previous studies conducted with 2-D endothelial monolayer models suggested that the gamma irradiation treatment leads to endothelial cell injury as well as changes in the actin filament structures22. These changes in the actin filament structures were also observed in our 3-D endothelial barrier model. In the non-irradiated hMVEC monolayers, F-actin was locally expressed along the cell edge with a thin layer, and the actin bundles were clearly observed within the cytoplasm of the endothelial cells. However, 4 days after the gamma irradiation exposure, we can figure out that gamma irradiation exposure increases the proportion of hMVECs with a high content of stress fibers. In particular, for the hMVECs which were exposed to high dose (8 Gy) of gamma irradiation, significant changes in the proportion of cells with no stress fibers and over 10 stress fibers were observed (Fig. 2b, white arrows). In addition, it was also observed that the cell–cell contact was weakened (Fig. 2a, yellow arrows, Fig. S2).

Monitoring the cell migration of the hMVECs in the microfluidic after gamma irradiation

The main advantage of our 3-D blood vessel model is that it can develop well-defined chemical gradients and monitor the cellular behaviors in the 3-D ECM hydrogel. Our previous research demonstrated that the VEGF gradient attracted endothelial cells into the ECM, which mimics in vivo angiogenic sprouting32. In tumor microenvironments, tumors secrete a variety of growth factors in order to recruit new blood vessels (angiogenesis), which can determine the efficacy of tumor chemotherapy and radiotherapy. As a result, recent tumor therapies have targeted the removal of tumors and inhibited tumor vasculature.

To study the effect of gamma irradiation on endothelial angiogenesis, we utilized 3-D blood vessel barrier models as shown in “Endothelial barrier formation in a 3-D microfluidic chip” section. VEGF-A, which is a cytokine that attracts endothelial cells, was introduced to the side channels for an additional 5 days to develop the VEGF-A gradient between the central and side channels (Fig. 5a). We can observe that hMVECs with VEGF-A gradient migrated into the ECM hydrogel while almost none of cells were migrated without VEGF-A gradient. And, these VEGF-A induced cell migrations were also observed even after radiation exposure (Fig. S5). Although endothelial sensitivity to gamma irradiation differs according to the origin and types of endothelial cells, microvascular endothelial cells used in this paper are known to be radio-sensitive endothelial cell types39. Previous studies have demonstrated that gamma irradiation exposure suppresses angiogenesis in normal endothelial cells40. In our model, we also determined that the migration of hMVECs into the ECM hydrogel was suppressed in irradiated endothelial cells under a high-dose (8 Gy) irradiation (Fig. 5b). Moreover, the sprout morphology was clearly distinguished between non-irradiated and irradiated endothelial cells. Non-irradiated hMVECs actively migrated into the ECM hydrogel along the VEGF gradient and formed lumen structures. By contrast, the irradiated hMVECs revealed DLL4+ single cells that are scattered in the ECM discontinuously (Fig. 5c).

At this point, there are two factors that lead to abnormal sprouting. First, we previously confirmed that gamma irradiation exposure reduced the cell–cell junctions. The collective migration of the tip cells and the proliferative extension of the stalk cells are required in sprouting angiogenesis; they are largely affected by the cell junctions41,42. Thus, the weakened cell–cell junctions between the irradiated tip and the stalk cells can lead to the disruption of the stable integrity of these two cells. The next possible factor for suppressed angiogenesis in the irradiated hMVECs is the changes in the gene expression that regulate the cell behaviors and processes. By performing the qRT-PCR analysis, we can observe that the gene expressions of Notch1 and Jagged1 were up-regulated with high-dose (8 Gy) irradiation treated hMVECs (Fig. 5d). By contrast, the expression of Dll4 slightly decreased after the irradiation in comparison to the non-irradiated hMVECs.

It has been reported that Notch1 increases significantly with gamma irradiation and the notch signaling pathway is highly related to angiogenesis and the maturation of blood vessels43,44. Notch1 is regulated by its ligands Dll4 and Jagged1, which have opposing roles in angiogenesis. VEGF–VEGF receptor2 (VEGFR2) signaling, which is a key initiator of angiogenesis, induces Dll4 expression in the tip cells. In turn, Dll4 upregulates Notch1 expression and Dll4/Notch signaling reduces VEGFR2 expression in the neighboring stalk cells by inhibiting the tip cell selection. By contrast, Jagged1/Notch signaling acts as an antagonist to Dll4/Notch signaling by promoting the tip cell selection and sprouting. Likewise, the balance between these two notch signaling pathways is important for proper sprouting angiogenesis. However, the abnormally increased expression of Notch1 due to gamma irradiation exposure can lead to the dysfunction of endothelial cells to regulate the balance between tip and stalk cells, even under the VEGF stimuli.

Recent studies have proposed that the activation of Notch1 leads to the stabilization of the vessels by inhibiting the endothelial cell proliferation45. This means that the overexpression of Notch1 could inhibit the proliferation and reduce the filopodia extension of the stalk cells. In other words, although similar levels of tip cells migrated into the ECM hydrogel after the gamma irradiation exposure, the stalk cells cannot follow up the tip cells and form lumen structures (Fig. 5b, c). Of course, this defective angiogenesis can occur for the overexpression of Notch1 in irradiated endothelial cells as well as cell senescence due to DNA damage.

Conclusion

In this study, we proposed a 3-D blood vessel model for studying the radiation-induced defects in endothelial barrier functions and the angiogenic potential. Because blood vessels play a major role in supplying nutrients to tumors and determine tumor growth, or even regression after tumor therapy, many kinds of in vitro endothelial models have been used. However, little is known about the cellular behaviors of endothelial cells because of the limitations of conventional 2-D endothelial cell models, in which the interactions of the cell–cell or cell–extracellular matrix cannot be represented. As a result, the native characteristics of the blood vessel can be lost despite the convenience of the model. To overcome these drawbacks in the 2-D endothelial monolayer models, we introduced a 3-D blood vessel barrier model in a microfluidic chip. In our chip, the endothelial cells formed a tight and stable monolayer by remodeling the ECM hydrogel. After gamma irradiation (4 and 8 Gy), the number of apoptotic hMVECs was increased and the fiber structure of the hMVECs was reorganized. In addition, the reduction of tight junction protein Claudin 5 in irradiated hMVECs was significantly observed. These small defects in endothelial cells can affect the whole endothelium integrity and largely related to the increasing molecular permeability after gamma irradiation.

Furthermore, during tumor progression or regression after radiotherapy, tumors secrete growth factors or cytokines to recruit new blood vessels in a process called angiogenesis. However, in 2-D cell culture systems, it is difficult to apply the gradient of chemokines; in our 3-D microfluidic system, gradients can be maintained. In angiogenesis, the tip and stalk cells showed different cell phenotypes; the systematic serial migration of these cells is important for forming tight lumen structures during angiogenesis. However, it is difficult to distinguish the tip and stalk cells in 2-D monolayer models because these cells have a homogeneous phenotype. By contrast, these cell-specific behaviors can be easily observed in our 3-D vessel model. In effect, although several studies have reported that gamma irradiation exposure can suppress angiogenesis by showing changes in the gene expression, protein level, or coverage area, little is known about the changes in the behaviors of the tip and stalk cells. However, we can see that the migratory tip cells were reduced slightly after gamma irradiation. In addition, the major defect is that the stalk cells cannot follow the tip cells, and the endothelial cells cannot form tubes. This can be effectively visualized in terms of how the gamma irradiation affects the barrier functions and the angiogenesis of the endothelial cells. Therefore, we propose that our 3-D endothelial models can be applied to understand further the radiation-induced vascular changes by observing single endothelial cell behaviors within the ECM hydrogel. In addition, these advanced 3-D vessel models can be expanded to incorporate tumor cells or spheroids to investigate the interaction between the tumor and blood vessels after gamma irradiation exposure.

References

1. 1.

Herfarth, K. K. et al. Stereotactic single-dose radiation therapy of liver tumors: Results of a phase I/II trial. J. Clin. Oncol. 19, 164–170 (2001).

2. 2.

Chao, K. S. C. et al. Intensity-modulated radiation therapy for oropharyngeal carcinoma: Impact of tumor volume. Int. J. Radiat. Oncol. Biol. Phys. 59, 43–50 (2004).

3. 3.

Fayos, J. V. & Kim, Y. H. Radiation therapy of brain tumors. Cancer 45, 12–18 (1979).

4. 4.

Baskar, R., Lee, K. A., Yeo, R. & Yeoh, K. W. Cancer and radiation therapy: Current advances and future directions. Int. J. Med. Sci. 9, 193–199 (2012).

5. 5.

Delanian, S. & Lefaix, J. L. Current management for late normal tissue injury: Radiation-induced fibrosis and necrosis. Semin. Radiat. Oncol. 17, 99–107 (2007).

6. 6.

Popanda, O., Marquardt, J. U., Chang-Claude, J. & Schmezer, P. Genetic variation in normal tissue toxicity induced by ionizing radiation. Mutat. Res. Fundam. Mol. Mech. Mutagen. 667, 58–69 (2009).

7. 7.

Citrin, D. et al. Radioprotectors and mitigators of radiation-induced normal tissue injury. Oncologist 15, 360–371 (2010).

8. 8.

Hölscher, T., Bentzen, S. M. & Baumann, M. Influence of connective tissue diseases on the expression of radiation side effects: A systematic review. Radiother. Oncol. 78, 123–130 (2006).

9. 9.

Dachs, G. U. & Chaplin, D. J. Microenvironmental control of gene expression: Implications for tumor angiogenesis, progression, and metastasis. Semin. Radiat. Oncol. 8, 208–216 (1998).

10. 10.

Dvorak, H. F., Weaver, V. M., Tlsty, T. D. & Bergers, G. Tumor microenvironment and progression. J. Surg. Oncol. 103, 468–474 (2011).

11. 11.

Neitzel, L. T., Neitzel, C. D., Magee, K. L. & Malafa, M. P. Angiogenesis correlates with metastasis in melanoma. Ann. Surg. Oncol. 6, 70–74 (1999).

12. 12.

Quail, D. F. & Joyce, J. A. Microenvironmental regulation of tumor progression and metastasis. Nat. Med. 19, 1423–1437 (2013).

13. 13.

Maishi, N. & Hida, K. Tumor endothelial cells accelerate tumor metastasis. Cancer Sci. 108, 1921–1926 (2017).

14. 14.

Ritter, E. et al. Breast cancer cell-derived fibroblast growth factor 2 and vascular endothelial growth factor are chemoattractants for bone marrow stromal stem cells. Ann. Surg. 247, 310–314 (2008).

15. 15.

Tsuzuki, Y. et al. Vascular endothelial growth factor (VEGF) modulation by targeting hypoxia-inducible factor-1α → hypoxia response element → VEGF cascade differentially regulates vascular response and growth rate in tumors. Cancer Res. 60, 6248–6252 (2000).

16. 16.

Hendriksen, E. M. et al. Angiogenesis, hypoxia and VEGF expression during tumour growth in a human xenograft tumour model. Microvasc. Res. 77, 96–103 (2009).

17. 17.

Chouaib, S. et al. Hypoxia promotes tumor growth in linking angiogenesis to immune escape. Front. Immunol. 3, 1–10 (2012).

18. 18.

Hovinga, K. E. et al. Radiation-enhanced vascular endothelial growth factor (VEGF) secretion in glioblastoma multiforme cell lines—A clue to radioresistance?. J. Neurooncol. 74, 99–103 (2005).

19. 19.

Staehler, M. et al. Simultaneous anti-angiogenic therapy and single-fraction radiosurgery in clinically relevant metastases from renal cell carcinoma. BJU Int. 108, 673–678 (2011).

20. 20.

Goedegebuure, R. S. A., De Klerk, L. K., Bass, A. J., Derks, S. & Thijssen, V. L. J. L. Combining radiotherapy with anti-angiogenic therapy and immunotherapy; A therapeutic triad for cancer?. Front. Immunol. 10, 1–15 (2019).

21. 21.

Kim, K. S., Kim, J. E., Choi, K. J., Bae, S. & Kim, D. H. Characterization of DNA damage-induced cellular senescence by ionizing radiation in endothelial cells. Int. J. Radiat. Biol. 90, 71–80 (2014).

22. 22.

Gabryś, D. et al. Radiation effects on the cytoskeleton of endothelial cells and endothelial monolayer permeability. Int. J. Radiat. Oncol. Biol. Phys. 69, 1553–1562 (2007).

23. 23.

Wang, Y., Boerma, M. & Zhou, D. Ionizing radiation-induced endothelial cell senescence and cardiovascular diseases. Radiat. Res. 186, 153–161 (2016).

24. 24.

Wagner-Ecker, M., Schwager, C., Wirkner, U., Abdollahi, A. & Huber, P. E. MicroRNA expression after ionizing radiation in human endothelial cells. Radiat. Oncol. 5, 1–10 (2010).

25. 25.

Baselet, B., Sonveaux, P., Baatout, S. & Aerts, A. Pathological effects of ionizing radiation: Endothelial activation and dysfunction. Cell. Mol. Life Sci. 76, 699–728 (2019).

26. 26.

Kouam, P. N., Rezniczek, G. A., Adamietz, I. A. & Bühler, H. Ionizing radiation increases the endothelial permeability and the transendothelial migration of tumor cells through ADAM10-activation and subsequent degradation of VE-cadherin. BMC Cancer 19, 958 (2019).

27. 27.

Wang, H. et al. Gamma radiation-induced disruption of cellular junctions in HUVECs is mediated through affecting MAPK/NF—κ B inflammatory pathways. Oxid. Med. Cell. Longev. 2019, 1–13 (2019).

28. 28.

Pampaloni, F., Reynaud, E. G. & Stelzer, E. H. K. The third dimension bridges the gap between cell culture and live tissue. Nat. Rev. Mol. Cell Biol. 8, 839–845 (2007).

29. 29.

Justice, B. A., Badr, N. A. & Felder, R. A. 3D cell culture opens new dimensions in cell-based assays. Drug Discov. Today 14, 102–107 (2009).

30. 30.

Duval, K. et al. Modeling physiological events in 2D vs. 3D cell culture. Physiology 32, 266–277 (2017).

31. 31.

Han, S. et al. Constructive remodeling of a synthetic endothelial extracellular matrix. Sci. Rep. https://doi.org/10.1038/srep18290 (2015).

32. 32.

Jeong, G. S. et al. Sprouting angiogenesis under a chemical gradient regulated by interactions with an endothelial monolayer in a microfluidic platform. Anal. Chem. 83, 8454–8459 (2011).

33. 33.

Kihara, T., Ito, J. & Miyake, J. Measurement of biomolecular diffusion in extracellular matrix condensed by fibroblasts using fluorescence correlation spectroscopy. PLoS ONE 8, e82382 (2013).

34. 34.

Kluger, M. S., Clark, P. R., Tellides, G., Gerke, V. & Pober, J. S. Claudin-5 controls intercellular barriers of human dermal microvascular but not human umbilical vein endothelial cells. Arterioscler. Thromb. Vasc. Biol. 33, 489–500 (2013).

35. 35.

Schnittler, H. et al. Actin filament dynamics and endothelial cell junctions: The Ying and Yang between stabilization and motion. Cell Tissue Res. 355, 529–543 (2014).

36. 36.

Schnittler, H. J. et al. Role of actin filaments in endothelial cell-cell adhesion and membrane stability under fluid shear stress. Pflugers Arch. Eur. J. Physiol. 442, 675–687 (2001).

37. 37.

Prasain, N. & Stevens, T. The actin cytoskeleton in endothelial cell phenotypes. Microvasc. Res. 77, 53–63 (2009).

38. 38.

Greene, C., Hanley, N. & Campbell, M. Claudin-5: Gatekeeper of neurological function. Fluids Barriers CNS 16, 1–15 (2019).

39. 39.

Park, M. T., Oh, E. T., Song, M. J., Lee, H. & Park, H. J. Radio-sensitivities and angiogenic signaling pathways of irradiated normal endothelial cells derived from diverse human organs. J. Radiat. Res. 53, 570–580 (2012).

40. 40.

Tsai, J. H. et al. Ionizing radiation inhibits tumor neovascularization by inducing ineffective angiogenesis. Cancer Biol. Ther. 4, 1395–1400 (2005).

41. 41.

Chen, W. et al. The endothelial tip-stalk cell selection and shuffling during angiogenesis. J. Cell Commun. Signal. 13, 291–301 (2019).

42. 42.

Blanco, R. & Gerhardt, H. VEGF and notch in tip and stalk cell selection. Cold Spring Harb. Perspect. Med. 3, 1–19 (2013).

43. 43.

Lobov, I. & Mikhailova, N. The role of Dll4/notch signaling in normal and pathological ocular angiogenesis: Dll4 controls blood vessel sprouting and vessel remodeling in normal and pathological conditions. J. Ophthalmol. 2018, 1–8 (2018).

44. 44.

Siekmann, A. F. & Lawson, N. D. Notch signalling and the regulation of angiogenesis. Cell Adhes. Migr. 1, 104–105 (2007).

45. 45.

MacK, J. J. & Iruela-Arispe, M. L. NOTCH regulation of the endothelial cell phenotype. Curr. Opin. Hematol. 25, 212–218 (2018).

Acknowledgements

This work was supported by the Korea Evaluation Institute of Industrial Technology (KEIT) Grant funded by the Korea government (MSIT) (20009125). Seok Chung was supported by the National Research Foundation of Korea (NRF) Grant funded by the Korea government. (MSIT) (2020R1A2B5B03002005). Ji-hun Yang was supported by the Ministry of Trade, Industry & Energy (MOTIE, Korea) (20009853) and the KIST Institutional Program (2E29200-19-004).

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K.N. (designed the study, performed experiments, analysed and interpreted results and wrote the manuscript), Y.C. (performed computer simulation and participated in the discussion and interpretation of the data), D.-H.C. (participated in chip preparation and gamma irradiation treatment), M.-J.P. (helped in performing experiments), J.Y. and S.C. (participated in the discussion, reviewed and approved the manuscript). All authors reviewed the manuscript.

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Correspondence to Ji-hun Yang or Seok Chung.

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Na, K., Cho, Y., Choi, DH. et al. Gamma irradiation exposure for collapsed cell junctions and reduced angiogenesis of 3-D in vitro blood vessels. Sci Rep 11, 18230 (2021). https://doi.org/10.1038/s41598-021-97692-8

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