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In this paper a single particle/cell-tracking microfluidic device that integrates an out-of-plane multimode optical fiber (OP-MMF) is reported. This OP-MMF is used to generate three excitation light-lines and three detection spots using only one excitation source and one detector. It takes advantage of an optical tunneling mode to create two excitation lines in a microfluidic channel emanating from a single fiber end. This method was used to accurately count particles/cells and perform velocity measurements and size discrimination. The velocity and size distributions of 5, 7, and 10 μm fluorescently labeled polystyrene beads were determined using the OP-MMF. Additionally, this method was used to analyze cell lysates with the third excitation line in the separation channel. The OP-MMF setup accurately detected an intact cell twice ∼2 mm prior to lysis, determined its velocity, and detected the injected cell lysate 3 mm downstream of the injection point in the separation channel. Using this setup, the velocity of cells entering the lysis intersection and the absolute migration times of fluorescently labeled analytes injected into the separation channel were determined in an automated fashion. This method enabled us to determine a lysing/injection efficiency coefficient (K) using signals from the injected lysate signal and from the intact cell before lysing. K provided a reliable measurement of the amount of cell lysate that was injected into the separation channel. The approach reported here could be used in the future to track particles, cells or droplets in a variety of existing microfluidic devices without the need for multiplexed masks, layers, bulky optical elements or complex optical designs.

A microfluidic device is reported that employs an out-of-plane optical fiber bridge to generate two excitation and two detection spots in a microfluidic channel using only one excitation source and one detector. This fiber optic bridge was integrated into a single cell analysis device to detect an intact cell just prior to lysis and the injected lysate 2, 5, 10, or 15 mm downstream of the injection point. Using this setup the absolute migration times for analytes from cells stochastically entering the lysis intersection could be determined for the first time in an automated fashion. This allowed the evaluation of several separation parameters, including analyte band velocity, migration time drift, diffusion coefficient, injection plug length, separation efficiency (N), and plate height (H), which previously could only be estimated. To demonstrate the utility of this system, a peptide substrate for protein kinase B (PKB) was designed, synthesized, and loaded into T-lymphocytes in order to measure PKB activity in individual cells. The optical fiber bridge is easy to implement, inexpensive, and flexible in terms of changing the distances between the two detection points.

The ability to accurately control fluid transport in microfluidic devices is key for developing high-throughput methods for single cell analysis. Making small, reproducible changes to flow rates, however, to optimize lysis and injection using pumps external to the microfluidic device are challenging and time-consuming. To improve the throughput and increase the number of cells analyzed, we have integrated previously reported micropumps into a microfluidic device that can increase the cell analysis rate to ∼1000 cells/h and operate for over an hour continuously. In order to increase the flow rates sufficiently to handle cells at a higher throughput, three sets of pumps were multiplexed. These pumps are simple, low-cost, durable, easy to fabricate, and biocompatible. They provide precise control of the flow rate up to 9.2 nL/s. These devices were used to automatically transport, lyse, and electrophoretically separate T-Lymphocyte cells loaded with Oregon green and 6-carboxyfluorescein. Peak overlap statistics predicted the number of fully resolved single-cell electropherograms seen. In addition, there was no change in the average fluorescent dye peak areas indicating that the cells remained intact and the dyes did not leak out of the cells over the 1 h analysis time. The cell lysate peak area distribution followed that expected of an asynchronous steady-state population of immortalized cells., (© 2016 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim.)

A considerable amount of attention has been focused on the analysis of single cells in an effort to better understand cell heterogeneity in cancer and neurodegenerative diseases. Although microfluidic devices have several advantages for single cell analysis, few papers have actually demonstrated the ability of these devices to monitor chemical changes in perturbed biological systems. In this paper, a new microfluidic channel manifold is described that integrates cell transport, lysis, injection, electrophoretic separation, and fluorescence detection into a single device, making it possible to analyze individual cells at a rate of 10 cells/min in an automated fashion. The system was employed to measure nitric oxide (NO) production in single T-lymphocytes (Jurkat cells) using a fluorescent marker, 4-amino-5-methylamino-2',7'-difluorofluorescein diacetate (DAF-FM DA). The cells were also labeled with 6-carboxyfluorescein diacetate (6-CFDA) as an internal standard. The NO production by control cells was compared to that of cells stimulated using lipopolysaccharide (LPS), which is known to cause the expression of inducible nitric oxide synthase (iNOS) in immune-type cells. Statistical analysis of the resulting electropherograms from a population of cells indicated a 2-fold increase in NO production in the induced cells. These results compare nicely to a recently published bulk cell analysis of NO.