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Journal of Nanomaterials
Volume 2015, Article ID 391850, 6 pages
http://dx.doi.org/10.1155/2015/391850
Research Article

Preparation of Homogeneous Nanostructures in 5 Minutes for Cancer Cells Capture

1Department of Oncology, The Second Affiliated Hospital of Southeast University, Nanjing, Jiangsu 210003, China
2The Fourth Clinical Medical College of Nanjing Medical University, Nanjing, Jiangsu 210009, China
3Department of Radiation Oncology, The Affiliated Jiangsu Cancer Hospital of Nanjing Medical University, Nanjing, Jiangsu 210009, China

Received 30 December 2014; Revised 28 March 2015; Accepted 31 March 2015

Academic Editor: Yaling Liu

Copyright © 2015 Lixue Wang et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Grafting aptamers on nanostructured substrates has shown ultrasensitivity in isolation of circulating tumor cells (CTCs). Here, we report that over 80 cm2 of homogenous nanostructured surface on glass substrates can be prepared in 5 min after one-step dry etching. The surface area was doubled; the average diameter of nanostructures is approximately 374 nm, which is more close to the nanostructures of natural extracellular matrix. Antiepithelial cell adhesion molecule aptamers grafted nanostructured glass substrates captured over 76% of PC3 cells compared to 30% of planar substrates. Bispecific aptamers cofunctionalized nanostructured substrates, however, fail to capture cancer cells probably due to the formation of heterodimers. This limitation reveals that multispecific aptamers, when applied to cell isolation, must be analyzed to exclude any potential formation of heterodimers due to complementary sequence matching.

1. Introduction

Circulating tumor cells (CTCs) as emerging tumor biomarkers can provide valuable information for clinical diagnosis, prognosis, and treatment [15]. Over the last decade, numerous methods for detection and isolation of CTCs have been developed [6]. Recently, nanostructured substrates have emerged as very promising tools. They provide more surface area for ligands immobilization and lower the rolling velocity of cells in microchannels [7, 8]. Cancer cells also can dynamically arrange focal adhesion points [9]. However, there are two major challenges. First, due to the limitations of existing nanofabrication techniques, large-scale fabrication of homogeneous nanostructured substrates is nontrivial [10, 11]. These nanostructured substrates in small pieces (few cm2) only process a limited amount of blood at a time (≤1 mL) [1]. Clinically relevant CTCs detection approaches should be able to process at least 7.5 mL of blood [12]. Thus, preparation of homogeneous nanostructures in large area is compulsory. Heterogeneity of CTCs poses the other challenge. Currently biological isolation approaches heavily rely on antiepithelial cell adhesion molecule (EpCAM). However, CTCs may have little or no expression of EpCAM on the cell membrane [13], causing biased isolation of CTCs [14].

To prepare homogeneous nanostructures in larger area, we develop a new recipe using C3F8 and C4F8 as etchant gas and successfully obtain approximately 80 cm2 projected area of homogeneous nanostructures after one-step dry etching in 5 min. Such area theoretically can process 8 mL whole blood samples for detection of CTCs [15]. On the other hand, to alleviate the challenge raised by heterogeneity of CTCs, we immobilize bispecific aptamers on nanostructured glass surface for cancer cells isolation. Aptamers are single-stranded oligomers that can specifically recognize and bind to target protein [16]. They are chemically stable at a wide range of pH, temperature, and ionic conditions [17]. Moreover, aptamers can be prepared in large quantity without batch-to-batch variation [18]. Bispecific aptamers have been used for targeted drug delivery [19]. However, it is unknown whether bispecific aptamers are able to increase isolation efficiency of cancer cells yet. To test the isolation efficiency, anti-EpCAM aptamers (AEA) or antiprostate specific membrane antigen (PSMA) aptamers (APA) are used.

Our results show that nanostructures with diameters ranging from 127 to 413 nm are successfully prepared, and nanostructured substrates can significantly increase cell capture efficacy. However, bispecific aptamers of AEA/APA mixture fail to capture PC3 cells due to the potential formation of heterodimers.

2. Materials and Methods

All chemicals were obtained from Sigma-Aldrich unless otherwise noted.

2.1. Glass Slides Etching and Characterization

The glass slides (Borofloat 33, Schott) were cleaned in piranha solution for 10 min at 90°C., followed by rinsing with DI water and drying in nitrogen flow. To create nanostructured surfaces, plain glass surface was subjected to RIE (ULVAC, NLD570 oxide etcher) for 3 to 15 min. The RIE condition was selected as C3F8 (30 sccm), C4F8 (10 sccm), Ar (50 sccm), O2 (10 sccm), antenna power (2000 W), bias power (50–200 W), and chamber pressure (5 mTorr). After the RIE process, the glass surface was cleaned using piranha solution and DI water. Surface topography was evaluated quantitatively using a JPK atomic force microscope (AFM). Images of 10 × 10 μm area were captured in tapping model.

2.2. Cell Culture

PC3 cells (EpCAM+/PSMA) were cultured in DMEM supplemented with 10% FBS, penicillin:streptomycin 100 U/mL and plated in T-25 tissue culture flasks (Corning, US). Flasks were placed into an incubator maintaining 5% CO2 at 37°C and 10% humidity.

2.3. Aptamers Binding to Cancer Cells

The respective sequences of AEA and APA (Sangon, Shanghai) were shown in Table 1. To confirm the binding of aptamer to cancer cells, Cy3 fluorescent groups labelled AEA, APA, and control DNA were incubated with PC3 cells. The aptamers were denatured by heating samples to 70°C for 5 minutes and then slowly cooling to RT. Cells in duplicate were seeded into 6-well cell culture plate and cultured for 48 hours. The aptamers and control DNA were incubated with cells at 37°C for 30 minutes under 5% CO2. After incubation, the cells were washed with 1x PBS three times, fixed with 4% paraformaldehyde for 30 min, and then stored in 1x PBS for optical and fluorescence imaging. The fluorescence images were taken followed by analysis of fluorescence intensity with ImageJ.

Table 1: Sequences of respective aptamers and control DNA.
2.4. Immobilize Aptamers onto Nanostructured Glass Surface

All glass samples were immersed in 5% 3-aminopropyltriethoxysilane (APTES) in ethanol for 2 h at RT. The silanized substrates were then sequentially rinsed with DI water and cured at 120°C for 1 h. The substrates were then immersed in a dimethylformamide (DMF) solution containing 10% pyridine and 1 mM phenyldiisothiocyanate (PDITC) for 2 hours. Each substrate was then washed sequentially with DMF and 1,2-dichloroethane and dried under a stream of nitrogen. The amine group modified aptamers were prepared at 30 μM in DI water (ratio of AEA/APA: 1 : 3, 1 : 1, and 3 : 1). A volume of 25 μL of aptamer solution was placed on each substrate and allowed to incubate in a humidity chamber at 37°C overnight. Each substrate was then sequentially washed with methanol and DI water. The functionalized surface was then deactivated by capping unreacted PDITC moieties by immersion in 50 mM 6-amino-1-hexanol in DMF for 5 hours. Each substrate was then sequentially rinsed with DMF, methanol, and DI water.

2.5. Cell Capture Assay and Image Analysis

Four devices functionalized with AEA, APA, AEA/APA, and control DNA, respectively, were prepared for each type of cell. 1 × 105 cells/mL 500 μL of cell suspension was seeded onto 1 × 1 cm device surface and incubated at 37°C for 30 min, and then 1x PBS was used to wash off the nonspecifically bound cells. Captured cells were fixed with 4% paraformaldehyde for 1 h at RT and then treated with permeabilizing block buffer (1x PBS with 0.5% sodium azide supplemented with 0.05% Triton X-100 and 10% BSA). Cells were then washed with perm wash 1x PBS supplemented with 0.5% sodium azide followed by 0.1 μg/mL DAPI staining. The whole glass slide was analyzed using Cytell (GE, US) high-content imaging system using 10x objectives. The number of captured cells was counted through DAPI stained nuclei of cells. Cell capture efficiency was then defined as the ratio of the number of captured cells to the total number of cells.

2.6. Electrophoresis Analysis of Heterodimers

8 μL of AEA and 8 μL of APA at 50 pM in 1x PBS were well mixed and denatured at 95°C for 5 min and then slowly cooled to RT. 8 μL of AEA or APA at 50 pM in 1x PBS was treated by the same procedure. Samples were analyzed by 4% agarose gel electrophoresis at 80 V at 4°C.

3. Results and Discussion

3.1. Characterization of Nanostructures

AFM images of samples and quantified results are shown in Figure 1 and Table 2. The increase of bias power can significantly increase the surface roughness. High bias power (200 W) is not ideal for preparation of homogeneous nanostructures and thus is excluded. Insular and abrupt microstructures are found probably due to fast etching rate (Figure 1(d)). We choose 100 W bias power and treatment for 5 min in following experiments. Previous research validated that cancer cell capture yield increased with nanoroughness [9]. Roughness of 203 nm obtained at 100 W is better. Moreover, the mean diameter of nanostructures obtained at 100 W for 5 min is 374.3 nm (Figure 1(c)). The size is more close to the nanostructures of natural extracellular matrix which fall in the range of 260 to 410 nm [1].

Table 2: Characterization of glass substrates under different etching conditions.
Figure 1: AFM images (10 × 10 μm2) of the surface roughness of etched glass. (a) shows glass surface before etching; (b) shows glass etched at 50 W for 5 min; (c) shows glass etched at 100 W for 5 min; (d) shows glass etched at 200 W for 5 min.
3.2. Aptamers Binding to Cancer Cells

To confirm AEA and APA can specifically recognize and bind to PC3 cells, Cy3 labelled AEA, APA, and control DNA were directly incubated with cells. The fluorescence intensity of respective aptamers is shown in Figure 2. The fluorescence signals reveal that AEA can bind to PC3 cells that weakly express EpCAM. Previous study has confirmed that APA can specifically recognize and internalize into PSMA+ cells with minimal uptake into PSMA PC3 cells [20]. We did not detect fluorescent signals from dye labelled APA because of null expression of PSMA on PC3 cell membrane. Nonspecific adsorption or binding of control DNA probes did not occur.

Figure 2: Average fluorescence intensity of AEA or APA binding to the LNCaP cells. Aptamers were allowed to interact and bind to cells at 37°C for 30 min in 5% CO2. After binding, the cells were washed with 1x PBS three times.
3.3. Cancer Cells Capture

We firstly compared the difference of capture yield of PC3 cells between planar and nanostructured substrates (Figure 3(a)). 30.4% (SD: 3.6%) and 76.2% (SD: 8.5%) of PC3 cells were captured on planar and nanostructured glass substrates with AEA, respectively. The low capture efficiency of AEA functionalized planar surface might be raised by the inherent low-affinity interactions of aptamers [21]. The dissociation constant () value of anti-EpCAM aptamer is approximately 20 nM, and it is fluctuant depending on the types of target cells [22]. Moreover, low amount of EpCAM (51,667 EpCAM molecules per cell) may be unable to gain sufficient binding forces during washing procedure [23]. In contrast, AEA grafted nanostructured substrates increase capture yield through higher odds of binding and higher total binding forces between AEA and EpCAM. In control groups, 1.4% (SD: 0.3%) and 0.5% (SD: 0.2%) of cells were captured on control DNA grafted planar and nanostructured substrates, respectively. Because PC3 cells do not express PSMA on cell membrane, approximately 1.2% (SD: 0.4%) and 0.7% (SD: 0.2%) of cells were nonspecifically captured onto APA functionalized planar and nanostructured substrates, respectively. Together, AEA grafted nanostructured substrates show better cell capture yield compared to that of planar substrates.

Figure 3: (a) shows average capture efficiency of PC3 cells on the AEA, APA, or AEA/APA functionalized planar and nanostructured surfaces; (b) shows differentiated capture efficiency of PC3 cells on the mixture of AEA and APA in ratio, respectively. 1 × 105 cells were seeded onto surfaces and incubated at 37°C for 30 min in 5% CO2. After binding, the cells were washed with 1x PBS three times.

Once we incubated PC3 cells on AEA/APA cofunctionalized planar and nanostructured substrates, cell capture yield decreased significantly. Only 8.2% (SD: 4.9%) and 6.7% (SD: 5.1%) PC3 cells were captured on planar and nanostructured substrates, respectively. It might be caused by heterodimer between AEA and APA. Further, we used mixed AEA/APA in different ratios (1 : 3, 1 : 1, and 3 : 1) to reveal the potential formation of heterodimers. PC3 cells capture yields were 0.5%, 6.7%, and 42.1%, respectively. If AEA and APA did not form any heterodimers, AEA/APA (3 : 1) theoretically could capture approximately 60% of PC3 cells. However, in practical experiments, only 42% of cells were captured by AEA/APA in 3 : 1 ratio. The results indicated that a number of AEA were unable to form suitable tertiary structures and to participate into antigens reorganization and capture. Alternatively, AEA does form right hairpin structures, but the recognition parts may be blocked by APA. However, in our design, both AEA and APA have 12 nt polyA spacer that can effectively prevent steric effect. Thus, the later speculation is invalid. The heterodimer analysis of AEA/APA and hairpin analysis of AEA or APA (IDT OligoAnalyzer 3.1) show the lowest Delta G value is −8.09, −4.08, and −4.87 kcal/mole, respectively. The values indicate all reactions are exergonic and spontaneous, and the heterodimer reaction between AEA and APA is more favourable. Figure 4 shows electrophoresis results of 16 μL of AEA/APA, 8 μL of APA, and 8 μL of AEA, respectively, at 15 and 30 min timepoint, respectively. If heterodimers do not exist, the mixture should show the exact same bands with that of AEA. Although an approximately 120-nt band appeared in both AEA and the mixture of AEA and APA, it is much weaker in the mixture. We speculate that, in the mixture, AEA and APA may form heterodimers after annealing. The continuous electrophoretic forces in 30 min gradually destroy these heterodimers [20, 21], and once AEA and APA are compulsorily separated the mixture begins to show the similar distribution of bands. We admit that we do not have direct evidences to confirm the heterodimers; nevertheless the electrophoresis results demonstrate that AEA and APA have mutual interactions that can impede their dissociation.

Figure 4: The potential heterodimer structure between AEA and APA. Electrophoresis of AEA, APA, and annealed AEA/APA at 15 and 30 min timepoints, respectively; samples were analyzed by 4% agarose gel electrophoresis at 80 V at 4°C.

4. Conclusion

Homogeneous nanostructures in approximately 370 nm diameter can reliably and quickly be prepared on borosilicate glass slides using our recipe, and the aptamer functionalized nanostructured substrates can significantly improve cancer cell capture yield. However, bispecific aptamers cografted surface failed to capture cancer cells probably due to the formation of heterodimers. The potential shortcoming may impair the application of multispecific aptamers for detection and isolation of molecules unless the heterodimers between selected aptamers can be strictly excluded.

Conflict of Interests

The authors declare no competing financial interests.

Authors’ Contribution

Lixue Wang and Chuandong Zhu contributed equally to this paper.

Acknowledgments

This project was supported by the Research Foundation of Jiangsu Provincial Commission of Health and Family Planning, China (Grant no. H201440); Medical Science and Technology Development Foundation, Nanjing Department of Health (Grant no. YKK14152); Jiangsu Provincial Natural Science Fund (no. BK20141018); “333” Project of Jiangsu Province (no. BRA2013292), Six Major Talent Peak Project of Jiangsu Province (class B, no. WS-047); and the Natural Science Foundation of China (nos. 30670619, 81072017).

References

  1. L. Wang, W. Asghar, U. Demirci, and Y. Wan, “Nanostructured substrates for isolation of circulating tumor cells,” Nano Today, vol. 8, no. 4, pp. 374–387, 2013. View at Publisher · View at Google Scholar · View at Scopus
  2. H. J. Yoon, M. Kozminsky, and S. Nagrath, “Emerging role of nanomaterials in circulating tumor cell isolation and analysis,” ACS Nano, vol. 8, no. 3, pp. 1995–2017, 2014. View at Publisher · View at Google Scholar · View at Scopus
  3. X. Liu and S. Wang, “Three-dimensional nano-biointerface as a new platform for guiding cell fate,” Chemical Society Reviews, vol. 43, no. 8, pp. 2385–2401, 2014. View at Publisher · View at Google Scholar · View at Scopus
  4. M. Lin, J.-F. Chen, Y.-T. Lu et al., “Nanostructure embedded microchips for detection, isolation, and characterization of circulating tumor cells,” Accounts of Chemical Research, vol. 47, no. 10, pp. 2941–2950, 2014. View at Publisher · View at Google Scholar
  5. H. Ma, J. Liu, M. M. Ali et al., “Nucleic acid aptamers in cancer research, diagnosis and therapy,” Chemical Society Reviews, vol. 44, no. 5, pp. 1240–1256, 2015. View at Publisher · View at Google Scholar
  6. M. Yu, S. Stott, M. Toner, S. Maheswaran, and D. A. Haber, “Circulating tumor cells: approaches to isolation and characterization,” The Journal of Cell Biology, vol. 192, no. 3, pp. 373–382, 2011. View at Publisher · View at Google Scholar · View at Scopus
  7. Y. Wan, M. A. I. Mahmood, N. Li et al., “Nanotextured substrates with immobilized aptamers for cancer cell isolation and cytology,” Cancer, vol. 118, no. 4, pp. 1145–1154, 2012. View at Publisher · View at Google Scholar · View at Scopus
  8. W. Han, B. A. Allio, D. G. Foster, and M. R. King, “Nanoparticle coatings for enhanced capture of flowing cells in microtubes,” ACS Nano, vol. 4, no. 1, pp. 174–180, 2010. View at Publisher · View at Google Scholar · View at Scopus
  9. W. Chen, S. Weng, F. Zhang et al., “Nanoroughened surfaces for efficient capture of circulating tumor cells without using capture antibodies,” ACS Nano, vol. 7, no. 1, pp. 566–575, 2013. View at Publisher · View at Google Scholar · View at Scopus
  10. S. Wang, Y. Wan, and Y. Liu, “Effects of nanopillar array diameter and spacing on cancer cell capture and cell behaviors,” Nanoscale, vol. 6, no. 21, pp. 12482–12489, 2014. View at Publisher · View at Google Scholar
  11. M. A. I. Mahmood, Y. Wan, M. Islam et al., “Micro+nanotexturing of substrates to enhance ligand-assisted cancer cell isolation,” Nanotechnology, vol. 25, no. 47, Article ID 475102, 2014. View at Publisher · View at Google Scholar
  12. J. C. Fischer, D. Niederacher, S. A. Topp et al., “Diagnostic leukapheresis enables reliable detection of circulating tumor cells of nonmetastatic cancer patients,” Proceedings of the National Academy of Sciences of the United States of America, vol. 110, no. 41, pp. 16580–16585, 2013. View at Publisher · View at Google Scholar · View at Scopus
  13. A. M. Sieuwerts, J. Kraan, J. Bolt et al., “Anti-epithelial cell adhesion molecule antibodies and the detection of circulating normal-like breast tumor cells,” Journal of the National Cancer Institute, vol. 101, no. 1, pp. 61–66, 2009. View at Publisher · View at Google Scholar · View at Scopus
  14. S.-M. Tu, “Heterogeneity of cancer,” in Origin of Cancers, pp. 129–136, Springer, Berlin, Germany, 2010. View at Google Scholar
  15. Y. Wan, M. Winter, B. Delalat et al., “Nanostructured polystyrene well plates allow unbiased high-throughput characterization of circulating tumor cells,” ACS Applied Materials & Interfaces, vol. 6, no. 23, pp. 20828–20836, 2014. View at Publisher · View at Google Scholar
  16. S. M. Nimjee, C. P. Rusconi, and B. A. Sullenger, “Aptamers: an emerging class of therapeutics,” Annual Review of Medicine, vol. 56, pp. 555–583, 2005. View at Publisher · View at Google Scholar · View at Scopus
  17. Y. Wan, J. Tan, W. Asghar, Y.-T. Kim, Y. Liu, and S. M. Iqbal, “Velocity effect on aptamer-based circulating tumor cell isolation in microfluidic devices,” The Journal of Physical Chemistry B, vol. 115, no. 47, pp. 13891–13896, 2011. View at Publisher · View at Google Scholar · View at Scopus
  18. Y. Wan, D. Tamuly, P. B. Allen et al., “Proliferation and migration of tumor cells in tapered channels,” Biomedical Microdevices, vol. 15, no. 4, pp. 635–643, 2013. View at Publisher · View at Google Scholar · View at Scopus
  19. G. Zhu, L. Meng, M. Ye et al., “Self-assembled aptamer-based drug carriers for bispecific cytotoxicity to cancer cells,” Chemistry, vol. 7, no. 7, pp. 1630–1636, 2012. View at Publisher · View at Google Scholar · View at Scopus
  20. O. Boyacioglu, C. H. Stuart, G. Kulik, and W. H. Gmeiner, “Dimeric DNA aptamer complexes for high-capacity-targeted drug delivery using ph-sensitive covalent linkages,” Molecular Therapy—Nucleic Acids, vol. 2, article e107, 2013. View at Publisher · View at Google Scholar · View at Scopus
  21. Y. Wan, Y.-T. Kim, N. Li et al., “Surface-immobilized aptamers for cancer cell isolation and microscopic cytology,” Cancer Research, vol. 70, no. 22, pp. 9371–9380, 2010. View at Publisher · View at Google Scholar · View at Scopus
  22. Y. Song, Z. Zhu, Y. An et al., “Selection of DNA aptamers against epithelial cell adhesion molecule for cancer cell imaging and circulating tumor cell capture,” Analytical Chemistry, vol. 85, no. 8, pp. 4141–4149, 2013. View at Publisher · View at Google Scholar · View at Scopus
  23. S. L. Stott, C.-H. Hsu, D. I. Tsukrov et al., “Isolation of circulating tumor cells using a microvortex-generating herringbone-chip,” Proceedings of the National Academy of Sciences of the United States of America, vol. 107, no. 43, pp. 18392–18397, 2010. View at Publisher · View at Google Scholar · View at Scopus