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Entropy 2015, 17(3), 1466-1476; doi:10.3390/e17031466
Abstract: While unique phenomena exist at fluid-solid phase intersections, many interfacial phenomena manifest solely on limited scales—i.e., the nm-μm ranges—which stifles their application potential. Here, we constructed microfluidic chips that utilize the unique long-distance interface effects of the Solute-Exclusion Zone (EZ) phenomenon to mix, separate, and guide samples in desired directions within microfluidic channels. On our “EZ Chip”, we utilized the interfacial force generated by EZs to transport specimens across streamlines without the need of an off-chip power source. The advantages of easy-integration, low fabrication cost, and no off-chip energy input make the EZ suitable for independent, portable lab-on-chip system applications.
The characteristic water molecular interactions within interfaces have been studied across a broad range of fields—e.g., nanoengineering, intracellular molecular motility, and protein folding. For instance, related research has revealed that reduced intracellular water mobility interoperated with polarized water layers formed within a cytoplasm [1,2]; ordered water molecules result in the oscillatory salvation force at liquid–solid interfaces [3,4]; and interfacial forces were applied for nanoparticle assembly . Moreover, structural water molecules may account for protein folding and may be involved in signal transductions in aquatic solutions [2,6,7]. Though hydrogen-bond water networks are widely recognized and appreciated on sub-micron scales, interfacial forces have not been fully explored for distances greater than one micrometer [2,4].
Solute-exclusion zones (EZs) were initially observed in the vicinity of hydrophilic surfaces . The discovery that water can form several-hundred-micron-thick, ordered layers when adjacent to hydrophilic surfaces—to effectively exclude colloidal particles and other solutes hundreds of microns from its surface—opened up promising interfacial water applications within the liquid-solid phase . Indeed, the concept of EZs prompted on-going investigation into novel applications of interfacial water. Within the EZ, microspheres were excluded ~600 μm from polymer surfaces at various velocities, depending on microsphere surface modifications ; macromolecules, such as pH indicator dyes, were excluded as well . The interfacial forces generated from EZs have been well documented [8,11] near diverse interfaces with various solvent parameters, such as ion concentrations and pH, where similar phenomenon have been reported [9,12].
Molecular dynamic simulations predicted the formation of a pseudo-crystal water lattice at polymer-water interfaces . Additionally, the hydration shell assembly and interfacial water clusters were proposed to interpret the formation of the exclusion force [2,14]. The energy stored within an EZ was investigated recently as well [15,16], and these studies confirmed the robust observations of EZ formation in the vicinity of various surfaces and interfaces. While the notable length scales of EZs range several hundred micrometers, herein, we applied EZ characteristics to perform basic manipulations, such as sorting, separation, and guided movement within microfluidic chip.
2. Results and Discussion
2.1. Observable Specimen Movements in Microfluidic Flow
We first demonstrated that the EZ force can drive the movement of samples in laminar flow within microchannels. Nafion 117, which has a carbon-fluorine backbone and hydrophilic perfluoro side-chains, was chosen to trigger EZ formation because it is an established means of doing so [8,11]. A straight microchannel was fabricated with Nafion 117 on one side opposite a side of acrylic polymers (Figure 1a). A specimen stream containing 0.5 μm carboxyl-functionalized fluorescent microspheres and a DI water stream were flowed through T-shaped inlets respectively, as indicated in Figure 1b.1. Here, we used a dashed line to represent the sample trajectory line. We observed that, in the presence of EZs, fluorescent microspheres moved perpendicular to the stream direction. Without off-chip energy input, our data showed that microspheres were continuously excluded from the Nafion surface (Figure 1b.2).
By changing channel geometry and flow rate, we demonstrated that the redistribution of microspheres was adjustable (Figures 1b.3 and 1b.4): In contrast to specimens transported at high velocity (~5 mm/s, Figure 1b.3), more microspheres were excluded into the DI stream at lower velocity (~0.5 mm/s, Figure 1b.4). In general, even when carried in dynamic water flow, specimens remained in an EZ. There are several alternative mechanisms in the established literature to explain the fundamental driving forces of EZs [9,11,17].
However, because our study focuses on the microfluidic applications of the EZ, it does not favor/support any particular EZ mechanism over another—and any discussion here of associated mechanisms remains speculative. Instead, our study focuses on applying the EZ to practical microfluidic manipulations. We consider that because the continuous flow passes the Nafion surface—where the microspheres stay in the EZ for only seconds—the contribution of gel dissolution and polymer brush effects can be eliminated in our system. Our data support that EZs exist in the laminar flow. We therefore can speculate that similar liquid-crystalline properties may contribute significantly to the EZ formation in dynamic flow . However, considering the high diffusion coefficient of monovalent ions, the contribution of diffusiophoresis in dynamic EZ formation should be considered as well . Indeed, additional studies are warranted to determine whether the laminar flow can carry the formed EZ structure, or whether EZs form dynamically during flow passing Nafion surfaces.
To evaluate particle movement using varying flow rates and flow path lengths, fluorescent microspheres that passed an EZ were collected from the T-shaped outlets. Microsphere concentrations were then quantified using spectrofluorophotometery. The EZ’s efficacy was evaluated by using:
Within microchannels, without active manipulations, cross-channel solute transportation is mainly dominated by diffusion, which is less efficient as solute size increases . In order to increase the efficiency, many active approaches have been developed, including methods such as electrokinetics, optical manipulation, and ultrasonic agitation [19,20]. However, the requirement of off-chip energy sources can greatly jeopardize the portability and self-sustainability of lab-on-chip systems . Our data support the potential capability of EZs to serve as embedded power sources, thereby presenting an alternative approach to microfluidic system operation. EZ Chips may serve as a starting point to build highly-flexible, easily-integrated, and low cost lab-on-a-chip devices—all without the need of an off-chip power source.
2.2. EZ Chip: Mixing, Separating, and Guiding
In this study, we expand on the solute-repelling capacity of the EZ to drive diverse sample manipulation. With specific microchannel designs, many fundamental “operation units” were included on our EZ Chips. When we considered the needs for clinical applications to assess dilute samples, the possibility of an EZ biological sample concentrator was examined (Figure 2a). To address this conceptually, fluorescent-labeled murine fibroblast cells were first suspended in Dulbecco’s phosphate buffered saline solution and then flowed into the EZ Chip.
Within the designed EZ concentrating region, the cells were excluded by EZs on both side channels. The result was an observable concentration of fibroblast cells in the middle of the microchannel within 30 s (Figure 2b).
Compared to abiotic samples—e.g., plastic microspheres and molecular dyes [8,9,11]—we demonstrated a proof of concept that EZ microfluidic effects may be applicable to biotic samples, which broadens the applications of EZs to clinic assays if additional attention is given to relevant parameters (e.g., survival rates). Therefore, because this experiment served only to demonstrate a biological concentrator conceptually, we speculate that future studies may determine if EZs can contribute to a range of mammalian cell assays. These studies can help determine, for instance, if EZs may be utilized to separate cells from serum in blood samples.
We then utilized EZ Chips to perform a widely-applied function: particle separation. Pre-mixed microspheres (diameters of 2 μm and 15 μm) were flowed through a fabricated EZ-sorter. To create the EZ-sorter, we utilized Nafion on one channel wall to generate an EZ across the channel (Figure 2c). A previous study demonstrated that microspheres with different diameters experience different exclusive forces in a static EZ . We confirmed similar results with our EZ-sorter: In laminar flow, we observed that 2 μm microspheres showed larger excluded movement than 15 μm microspheres. To quantify the separation efficiency, we used a nestled DI water stream to extract partitioned samples within the EZ (Figure 2c). The size distribution of microspheres collected from respective streams was analyzed using flow cytometry (LSR II, Becton Dickson, Franklin Lakes, NJ, USA). Compared to the 8% of 15 μm microspheres carried in Stream 1, only 2% of 15 μm microspheres were identified in Stream 2, which confirmed that the EZ-sorter functioned based on the microsphere size (Figure 2d). Compared to more developed sorting technologies—e.g., fluorescence activated cell sorting —EZ sorting by means of particle size remains limited in its application. However, when the values of cost efficiency and system portability are taken into account, a simple particle size EZ-sorter may serve as an effective disposable microfluidic system.
Various operation units, such as dielectrophoresis electrodes and surface acoustic waves , have been integrated into microfluidic chips to guide specimen transport. To further broaden the potential applications of EZs to microfluidic systems, we demonstrated a primary approach to specimen manipulation with an on-chip EZ. In this system, we aimed to transport microspheres from the main channel to the side reservoir, and switched the on-off states of the solute-exclusion by controlling flow rate. The Nafion was set up at the intersection of the main channel and the side-reservoir; microspheres were carried in the stream next to the Nafion surface, and another DI water stream was introduced to serve as a liquid boundary to prevent undesired microspheres from entering into the side-reservoir (Figure 3a). At a relatively high stream velocity (~1 mm/s), samples (0.5 μm fluorescent microspheres) passing the channel/reservoir intersection stayed in the main channel (Figure 3b-1–b-4). The transportation direction of microspheres was switched by the EZ once the stream velocity lowered to less than 150 μm/s. Time-lapse images showed the switch of microsphere movement; the microsphere flux started to cross the DI barrier to enter into the reservoir when the stream velocity was below 150 μm/s (Figure 3b-1 and Figure 3b-2). Once the stream velocity increased again, the samples in the reservoir were effectively trapped, isolated from samples in the main channel (Figure 3b-3 and 3b-4).
3. Experimental Section
Considering that an easily-accessed and low-cost fabrication process can facilitate the general use of microfluidic systems [22,23], in this study two methods that met these criteria were applied to fabricate the polymer-based EZ Chips. The first method was mechanical shearing. A low-cost mechanical shearing fabrication protocol, which provides sub-millimeter resolution, was applied to etch microchannels on polymer films directly . EZ Chips can be rapidly prototyped using this method, which also provides flexibility to fabricate microstructures on various polymeric materials. Nafion polymer sheets (Nafion 117, Sigma Aldrich, St. Louis, MO, USA), with their carbon-fluorine backbones and hydrophilic perfluoro side-chains, were chosen to trigger EZ formation because they are an established means of doing so [8,11].
In EZ Chips, double-sided tape (3M Crop, St. Paul, MN, USA) was chosen to serve as construction layers. Polydimethylsiloxane (PDMS, Sylgard 184 silicone elastomer kit, Dow Corning, Midland, MI, USA) was temporarily adhered to the top of the device as tubing connectors . In our second method, low-power laser (VesaLASER 2.30, Universal Laser systems, Scottsdale, AZ, USA), was used to address the desired EZ patterns in specific regions. This method allowed selective “deactivation” of the polymer surface (Figure 4a), as we observed that Nafion regions treated by the low-power laser lost the ability to form EZs adjacent to the treated surface. Laser scanning confocal microscopy was used to assess 3-dimensional EZs created by laser-patterned stripes on the Nafion surface. By suspending fluorescent microspheres in solution, we observed that specimens halted in the 200 μm-wide laser-patterned regions and formed clusters inversely correlated to the patterned surface (Figure 4b). This data suggested that, after Nafion surface deactivation, the Nafion surface lost the capacity to trigger EZs. Both methods provided high flexibility for EZ Chip designs and further extended the applications with a simple and low-cost fabrication processes.
In order to quantitatively monitor the exclusion ratio under different flow rates, stream velocities were controlled by a dual-channel syringe-pump (KD Scientific, Holliston, MA, USA). Fluorescent microspheres (Bangs Laboratories, Fishers, IN, USA) were used as representative samples, and the microsphere concentrations were quantified using spectrofluorophotometery (RF-1501, Shimadzu, Columbia, MD, USA). In summary, pre-mixed microsphere solution (sample-carry stream) and DI water were injected from individual inlets into EZ chip as indicated in Figure 1b.1. ~1 mL sample solutions passed EZ were collected separately into microcentrifuge tube for spectroflurophotometeric measurement.
The murine embryonic fibroblast cells (Millipore, Billerica, MA, USA) were used to study the possible applicability of the EZ Chip to biological sample assays. Before flowing into EZ Chips, cells were labelled with the Cell Tracker (CellTracker Red CMTPX, Invitrogen, Grand Island, NY, USA) for easy identification under the microscope. D-PBS and other cell culturing reagents were purchased from Invitrogen without specific indication. Images were acquired using epi-fluorescent microscopy (TE-2000, Nikon Instruments, Melville, NY, USA) and analyzed using image software (ImageJ, NIH, Bethesda, MD, USA).
We demonstrated how microfluidic chips (“EZ Chips”) may be manufactured to perform basic manipulations, such as sorting, separation, and guided movement within microfluidic channels. In doing so, we developed a laser ablation method for EZ Chip manufacturing. Among their many applications, microfluidic systems provide promising applications to diagnosis technologies . When we consider the dearth of reliable energy sources in resource-limited regions, low-cost, disposable, and self-sustained microfluidic chips seem critically needed. Without the need of off-chip energy input, we demonstrate the feasibility of utilizing the EZ phenomenon to drive microfluidic systems, which may serve to broaden the practical applications of microfluidic systems generally. EZs can be used to drive specimens within channels using carefully design patterns, only some of which were explored in this study. Here, we demonstrated the capacity to fabricate basic functional units on an EZ Chip. With our developing fabrication protocols, EZ units can be modified at desired locations to facilitate “operation unit” integration. Although our observations remain limited to specific functions, when we consider the simplicity and compartmentalized operations carried out by EZ Chips, we posit that future EZ Chips may carry additional potential to contribute to the next generation of disposable microfluidic systems.
This work was supported in part by grants from National Heart, Lung, and Blood Institute (1R15-HL-095039), National Science Foundation (CBET-0932404), Linkou Chang Gung Memorial Hospital (CMRPD1C0031), and University of California Center for Information Technology Research in the Interest of Society (UC CITRIS) Program.
Wei-Chun Chin and Chi-Shuo Chen conceived of the research subject of this paper. Erik Farr, Jesse Anaya, and Chi-Shuo Chen designed the microfluidics and carried out the experiments. Wei-Chun Chin, Chi-Shuo Chen, Jesse Anaya, and Erik Farr drafted the paper and approved the final version to be published. Wei-Chun Chin and Eric Chen contributed to the conception and critical suggestions of the paper. All authors have read and approved the final manuscript.
Conflicts of Interest
The authors declare no conflict of interest.
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