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In vitro testing of drug compounds on cell models during the drug development process represents an indispensable step in the initial screening process. Although drug testing on three-dimensional (3D) cultured cells may provide a more accurate prediction of drug efficacy, it is relatively costly and time-consuming to perform compared with conventional 2D cultures due to the thick z-axis of the 3D models. In this study, we have presented a microfluidic platform with integrated pneumatic valves for producing a thin-gel 3D cell culture-based combinatorial drug screening array (3D-μCDS array). The multilayer architecture and microfluidic layout has a smaller device footprint than a single-layer microfluidic channel arrangement, making it well suited to scaling up for high-throughput combinatorial drug screening on 3D cell model. We performed 8 × 8 combination drug screening experiments with the device using two anti-cancer drugs (doxorubicin and paclitaxel) on MDA-MB-231 and MCF-7 breast cancer cell lines for demonstration. Our results indicate that our 3D-μCDS array device allows the successful screening of multiple drug combinations while reducing the operation time and the number of sample/reagents required, making it an ideal tool for general combinatorial drug screening, as well as for applications using valuable tissues and clinical samples.

Neurosphere assay is a common and robust method for identification of neural stem/progenitor cells, but obtaining large numbers of live single cells from dissociated neurospheres is difficult using nonenzymatic methods. Here, we present an enzyme-free method for high-efficiency neurosphere dissociation into single cells using microfluidic device technology. This method allows single cell dissociation of DC115 and KT98 cells with high cell viabilities (80-85 %), single-cell yield (91-95 %), and recovery (75-93 %).

In vitro culture of single cells facilitates biological studies by deconvoluting complications from cell population heterogeneity. However, there is still a lack of simple yet high-throughput methods to perform single cell culture experiments. In this paper, we report the development and application of a microfluidic device with a dual-well (DW) design concept for high-yield single-cell loading (~77%) in large microwells (285 and 485 μm in diameter) which allowed for cell spreading, proliferation and differentiation. The increased single-cell loading yield is achieved by using sets of small microwells termed “capture-wells” and big microwells termed “culture-wells” according to their utilities for single-cell capture and culture, respectively. This novel device architecture allows the size of the “culture” microwells to be flexibly adjusted without affecting the single-cell loading efficiency making it useful for cell culture applications as demonstrated by our experiments of KT98 mouse neural stem cell differentiation, A549 and MDA-MB-435 cancer cell proliferation, and single-cell colony formation assay with A549 cells in this paper. [ABSTRACT FROM AUTHOR]

Single-cell cloning (SCC) is a critical step in generating monoclonal cell lines, which are widely used as in vitro models and for producing proteins with high reproducibility for research and the production of therapeutic drugs. In monoclonal cell line generation, the development time can be shortened by validating the monoclonality of the cloned cells. However, the validation process currently requires specialized equipment that is not readily available in general biology laboratories. Here, we report a disposable SCC device, in which single cells can be isolated, validated, and expanded to form monoclonal cell colonies using conventional micropipettes and microscopes. The monoclonal cells can be selectively transferred from the SCC chip to conventional culture plates, using a tissue puncher. Using the device, we demonstrated that monoclonal colonies of actin-GFP (green fluorescent protein) plasmid-transfected A549 cells could be formed in the device within nine days and subsequently transferred to wells in plates for further expansion. This approach offers a cost-effective alternative to the use of specialized equipment for monoclonal cell generation. [ABSTRACT FROM AUTHOR]