This work was supported by NSF PHY-1659940.

1. Fabrication of microfluidic device
<ol>
	<li>Generate the desired microfluidic pattern using a layout design software (see Supplemental Materials).</li>
	<li>Fabricate the photomask. See Table of Materials for more details.
	<ol>
		<li>Utilizing a laser writer, write the pattern on a soda-lime glass plate coated with 100 nm of Cr and 500 nm of photoresist AZ1518.</li>
		<li>Develop the photoresist with developer AZ300MIF for 60 s.</li>
		<li>Etch away the chromium without protection from the photoresist using Cr-7 Chromium Etchant.</li>
		<li>Strip off residual photoresist using a photoresist stripper at 70 &#176;C for 45 min.</li>
	</ol>
	</li>
	<li>Pattern the photoresist. See Table of Materials for more details.
	<ol>
		<li>Spin coat HMDS on silicon wafer at 4000 rpm for 40 s.</li>
		<li>Spin coat photoresist AZ4330 on silicon wafer at 4000 rpm for 40 s.</li>
		<li>Soft bake the silicon wafer at 95 &#176;C for 60 s.</li>
		<li>Utilize the mask aligner to expose UV to the silicon wafer.</li>
		<li>Develop the photoresist with developer AZ300MIF for 4 min.</li>
	</ol>
	</li>
	<li>Perform DRIE etching. See Table of Materials for more details.
	<ol>
		<li>Dry-etch the wafer patterned with the photoresist using a Silicon Deep Reactive Ion Etching (DRIE) system for 100 &#181;m depth.</li>
		<li>Strip off the photoresist with acetone and plasma etch with a plasma etcher.</li>
	</ol>
	</li>
	<li>Wafer oxidation and silanization. See Table of Materials for more details.
	<ol>
		<li>Perform thermal oxidation on the etched silicon wafer in a furnace at 1100 &#176;C for 1 h.</li>
		<li>Wait for the silicon wafer to cool down, and then place the wafer into a desiccator with a few drops of trichloro-1H,1H,2H,2H-perfluorooctyl-silane (PFOTS) dripped in a small container near the wafer.</li>
		<li>Pump the pressure of the desiccator to 0.5 atm at room temperature for 60 min. The silicon wafer mold should become hydrophobic after proper silanization, which can be tested by adding several droplets of water onto the wafer.</li>
	</ol>
	</li>
	<li>Soft lithography. See Table of Materials for more details.
	<ol>
		<li>Mix pre-polymer and cross-linker (from polymethylsiloxane (PDMS) kit) at a 10:1 by weight ratio.</li>
		<li>Pour the mixed PDMS to create a 10 mm film in height onto the silanized silicon wafer mold.</li>
		<li>Degas the resulting PDMS-silicon wafer system in a desiccator for 30 min to 1 h.</li>
		<li>Incubate the PDMS-silicon wafer in a 70 &#176;C incubator overnight to cure the PDMS.</li>
		<li>Once the PDMS is cured, peel the PDMS film off the silicon wafer carefully.</li>
		<li>Using biopsy needles, punch through-holes at the inlet ports based on the location of the pattern on the PDMS and employ a circular punch to cut chips 27 mm in diameter.</li>
	</ol>
	</li>
	<li>PDMS layer bonding.
	<ol>
		<li>Heat cure two stacks of 27 mm PDMS cylinders (without patterning), which will become the reservoir layer and the capping layer of the device.</li>
		<li>Cut out two 7 mm circles around the inlets on the reservoir layer, and utilize a biopsy needle to punch through-holes at the inlet ports on the capping layer.</li>
		<li>Bond three stacks of PDMS (patterned stack, reservoir layer, capping layer) with oxygen plasma treatment.</li>
		<li>With the biopsy needle, punch through-holes at the outlets and the center port of the device.</li>
	</ol>
	</li>
</ol>
2. Media and cell line preparation
<ol>
	<li>Prepare media for culturing PC3 cell lines, including PC3-EMT and PC3-EPI: mix RPMI 1640 medium with 10% fetal bovine serum (FBS) and 1x antibiotic-antimycotic. Generate cell lines as described previously14. 
	NOTE: PC3 cell lines are maintained in the above media in humidified incubators at 37 &#176;C with 5% CO2. Split cells and subculture every 3 days, before they reach 100% confluency.</li>
	<li>Transfect cell lines with cytoplasmic-labeled fluorescent markers for better visualization, as described previously12, such that PC3-EMT expresses cytoplasmic GFP and PC3-EPI expresses cytoplasmic mCherry. Note that the technology is also compatible with any fluorescent-labeled cells as well as brightfield imaging of unlabeled cells.</li>
</ol>
3. Experimental setup
<ol>
	<li>Fabrication of metal plate holder
	<ol>
		<li>Fabricate a plate holder that is sufficient to hold simultaneous gas-permeable culture dishes for parallel experiments by machining or 3D printing. The 3D CAD file (&#34;3-well plate.FCStd&#34;) can be found on GitHub as a reference (https://github.com/kechihl/3-well-plate).</li>
		<li>Unscrew the components of the holder (Figure 2) with a screwdriver. Disinfect the components via UV exposure for at least 1 h and leave in a sterile environment. 
		NOTE: The holder is designed to provide substantial conditions for thermal equilibrium and ideal gas compositions, with gas channel inlets that allow for airflow. More details can be found in our previous work12.</li>
		<li>Prepare up to three gas-permeable culture dishes, of which the cell culture membrane is relatively flexible.</li>
	</ol>
	</li>
	<li>Cell line seeding
	<ol>
		<li>24 hours before the start of the experiment, harvest PC3-EPI and PC3-EMT cells by trypsinization for 5 min. Add prewarmed culture media, then centrifuge at 150 x g for 3 min and discard the supernatant.</li>
		<li>Count cells of each PC3-EPI and PC3-EMT using a hemocytometer and isolate a total of 2.5 x 104 of each cell type for each gas-permeable culture dish.</li>
		<li>Mix and resuspend the two cell types in 2 mL of culture media and seed the cells into each of the gas-permeable culture dish.</li>
		<li>Leave the entire plate holder in the incubator overnight for cells to attach.</li>
		<li>Disinfect the PDMS devices via UV exposure for at least 1 h and leave in a sterile environment.</li>
	</ol>
	</li>
	<li>Setting up thermal control unit and gas supply system
	<ol>
		<li>As shown in Figure 3, set up a gas supply system that consists of both CO2 and O2 control units, a gas pump, a gas mixing chamber, a humidifier or bubbler, and three separate sets of gas valves and pressure gauges. More details can be found in our previous work12.</li>
		<li>Set up the CO2 and O2 control units such that they adjust the mixing rate of the gas from CO2 and N2 tanks and the O2 source. Alternatively, any gas supply system that provides gas under normoxia condition would work.</li>
		<li>Make sure the gas that is combined in the mixing chamber and humidified by a bubbler such that the relative humidity is increased up to 85% (as read out from a relative humidity monitor) and that the gas leads to three independent gas valves with pressure gauges in order to control and monitor gas flow rate in the plate holder.</li>
		<li>Place the entire plate holder in an on-stage incubation thermal control unit with separate heating subunits for the lid and the bottom plate, with all units set at 37 &#176;C. See Table of Materials for more details.</li>
	</ol>
	</li>
	<li>Installation of microfluidic device. See Table of Materials for more details.
	<ol>
		<li>Identify that the detailed components of the 3-well plate holder are in order, as in Figure 2. Each of the three wells are identical and independent, with a pair of gas channels for each well. Every well possesses a gas-permeable culture dish holder, a PDMS chip holder, a glass window holder, and a pair of 35 mm glass windows. These components can be assembled using the fitted screws. 
		NOTE: The glass windows ensure that there is a thermally-isolated space between the gas-permeable culture membrane and the well such that no water condensation occurs due to temperature differences at the interface. Note that the 3 wells are independent, and 3 experiments can be done separately.</li>
		<li>Pre-warm culture medium at 37 &#176;C and degas in a vacuum chamber for 20 min.</li>
		<li>Treat the PDMS chips using an oxygen plasma system for 30 s in order to maintain hydrophilicity.</li>
		<li>Set up the syringe system. Load two syringes slowly with growth media and other two syringes with desired reagent of interest (media, media with drug, etc.). Connect each individual syringe to a 50 cm tubing (0.020&#34; x 0.060&#34;OD) by a 23 G dispensing needle into one hollow steel pin. Insert a hollow steel pin into the other end of the tubing.</li>
		<li>Prime the tubing and insert the steel pin into each PDMS chip through the capping layer. Fill up the reservoir layer and wet the PDMS pattern layer pattern with media. The reservoir layer works as an on-chip bubble trap to prevent air bubbles from getting into the microfluidic pattern.</li>
		<li>Load a 1 mL syringe with culture media. Connect the syringe to a 5 cm tubing (0.020&#34; x 0.060&#34;OD) by a 23 G dispensing needle into one hollow steel pin. Insert a hollow steel pin into the other end of the tubing and prime the tubing.</li>
		<li>Insert the hollow steel pin into the center hole of the chip, where excessive media can be extracted out from the chip later during the chip sealing process.</li>
		<li>As each PDMS device requires four 10 mL syringes loaded onto a syringe pump, load two 10 mL syringes per chip in the forward deck. Place the two other syringes in the withdraw deck of the syringe system.</li>
		<li>Place chip directly on top of the gas-permeable culture membranes (with cells already adhered to the membranes). In order to avoid entrapping microbubbles in the microfluidic pattern, dispense 1 mL of prewarmed and degassed media into the 35 mm gas-permeable culture dish before assembly, and then make sure that the chip approaches the liquid surface with a 15-degree tilt angle.</li>
		<li>Clamp the gas-permeable culture dish and the well in the gas-permeable culture dish holder for each chip, with the PDMS chip holder pushing the PDMS device downward.</li>
		<li>Tape a sheet of a sealer on top of the PDMS device and clamp with the PDMS chip holder in order to prevent the chip from drying out.</li>
		<li>Set media flow rate around the array to be 20 &#181;L/h.</li>
		<li>Set the entire plate in the on-stage incubator on the motorized stage of an inverted microscope. Connect the gas supply system to the gas channels and pressurizing the gas-permeable culture membrane against the installed PDMS chip to ensure sealing of device. Maintain gauge pressure at 0.2 psi (1.4 x 104 Pa).</li>
		<li>Slowly extract excessive media in the chip using the 1-mL syringe from the center hole. Observe the chip under the microscope while extracting media and then stop extracting when the chip is sealed. Chip sealing should be obvious since a part of the cells would be crushed by the micro-structures.</li>
		<li>Connect the temperature sensing unit of the on-stage incubator to the 3-well plate and set to 37 &#176;C.</li>
	</ol>
	</li>
</ol>
4. Single-cell time-lapse imaging
<ol>
	<li>Set up imaging software utilizing an inverted microscope to time-lapse image acquisition. Note that an inverted fluorescent microscope with fully motorized x-y stage, focus knob, shutter, and filter cubes is required for an EA experiment.</li>
	<li>Configure software to acquire images across two channels at 10x magnification for each chip with automatic image-stitching after one round of autofocus. Be aware that automatic correction systems like Perfect Focus do not guarantee satisfying image quality. It is more recommended to generate a customized focus surface for long-term image acquisition based on either autofocus or manual focus across the chip.</li>
	<li>Take images every hour and leave experiment running on the time scale of weeks. Monitor image quality on a daily basis and update the focus surface if necessary.</li>
	<li>Prepare the PDMS chip and gas-permeable culture dish for subsequent immunofluorescent analysis, as described previously13.</li>
</ol>
5. Image processing and analysis
<ol>
	<li>Post-experimental processing
	<ol>
		<li>Convert images into TIFF format for image processing and measurements utilizing Fiji/ImageJ.</li>
		<li>Compress TIFF files for ease of further image processing.</li>
	</ol>
	</li>
	<li>Fiji/ImageJ analysis
	<ol>
		<li>To identify cells, perform Background Subtraction and Particle Analysis to identify fluorescent bright-spots for cell location detection and automatic cell counting.</li>
		<li>Utilize plugins (Manual Tracking, Chemotaxis, Migration Tool, Trackmate) to analyze cell motility and migration.</li>
	</ol>
	</li>
</ol>

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No conflicts of interest declared.

Conventional cell culture was developed almost a century ago and remains the most frequently used preclinical model in biomedical research, despite its proven limited ability to predict clinical results in cancer17. Animal models offer the highest physiological relevance and reasonable genetic similarity to humans, but have long been acknowledged to have significant limitations in predicting human outcomes18. Among all the existing preclinical models, microfluidic cancer-on-chip models appear to be the most promising candidate to satisfy the unmet need in cancer research9,19,20. However, current cancer-on-chip models have yet to offer a platform that is able to reproduce key components and interactions to mimic a tumor microenvironment in a comprehensive manner, yet simple enough to provide reliable and reproducible quantitative data. Our representative data demonstrate that our microfluidic cell culture technology provides stable physical and biochemical conditions for long-term cell culture in heterogeneous micro&#173;environments. This multifunctional platform allows the sophisticated adjustment of a time&#173;-dependent chemical gradient as well as ambient gas composition. The platform is portable and compatible to most of the fluorescent inverted microscopes for high&#173;-resolution real-time imaging, which offers multidimensional information of cells as a function of time, including cell morphology, population dynamics, cell motility and cell migration on a single-cell level.
Compared to our previous work11, we note that this pressure-sealing packaging and assembly method for our microfluidic device enables numerous downstream experiment capacities (e.g., FACS, local metabolite extraction, sub-clonal populations expansion, IF, DNA/RNA FISH, etc.) complementary to the time-lapse images taken in the course of the experiments. This capability of removing cells from specific locations in a heterogenous culture is a major advance compared to earlier devices, where the sealing surface to a chip had to be removed before one could access the culture11. Further, even in that case, the act of removing the cover significantly disturbed the culture so that local testing of cells on a single to few habitat levels was not possible. Such localized extraction was possible in our case due to the soft &#34;resealable&#34; nature of the flexible gas-permeable membrane.
There are several critical steps in the presented protocol. First of all, to initiate a long-term experiment with stable fluidic dynamics, microbubbles need to be avoided as much as possible. Therefore, it is important to prewarm and degas the culture medium (step 3.4.2) before loading the media into the syringes. The manipulation of media loading and dispensing should be done slowly and gently to prevent bubble formation. The PDMS pattern should be treated with oxygen plasma (step 3.4.3) before connecting to the culture media supply system. Oxygen plasma treatment ensures the hydrophilicity of the PDMS surface and significantly reduces the possibility of microbubble entrapping. In step 3.4.7., when placing the chip on top of the cell culture membrane, the PDMS chip should approach the liquid surface with a 15-degree tilt angle to get rid of the bubbles (if any) on the liquid surface inside the culture dish. Secondly, the pressure-sealing method requires a stable gas supply system that pressurizes the cell culture membrane. The pressure should be set between 0.2 to 0.6 psi. Pressure lower than 0.2 psi is insufficient for chip sealing. Above 1.2 psi, a significant amount of gas would permeate through the membrane and generate bubbles within the microfluidic pattern. We note that if the components of the metal 3-well plate are not properly assembled (including the plate body, the gas-permeable culture dish holder, a PDMS chip holder, a glass window holder, O-rings, and a pair of 35 mm glass windows), one would identify gas leakage as the pressure reading would be irresponsive to the increase of the gas flow. The leakage issue can be resolved simply by doing a leakage test and then reassembling the components.
The major form of data acquired with the utilization of the EA technology is through imaging. As mentioned previously, the EA technology can be installed on any inverted microscope. However, to fully exploit the advantages of the system, it is highly recommended to install the system on an inverted fluorescent microscope equipped with fully motorized x-y stage, motorized focus knob, motorized shutter, and motorized filter cube. Also, be aware that Perfect Focus might not guarantee satisfying image quality. We suggest using an imaging software that allows multi-dimensional image acquisition and customized imaging script. Keeping the images well-focused could be challenging without a periodic (every 24 hours or 48 hours) autofocus command, which generated a customized focus surface during the image acquisition cycle.
The presented microfluidic EA technology has been implemented to study the adaptation and evolution dynamics in prostate cancer cell metapopulations under a chemotherapeutic stress landscape12. We have also demonstrated the emergence of drug-resistance polyploid giant cancer cells in this tumor-like heterogeneous micro-ecology, showing that environmental heterogeneity combined with cell migration within tumor population would cause amplification on the emergence of resistant phenotypes13. With the ability to control and monitor the behaviors of mixed tumor cell populations under well-controlled stress gradients, our microfluidic EA technology may also serve as a platform to study regulatory mechanisms and the phenotypic transformation involved in EMT in the context of cancer therapeutic strategies21. Last but not least, the presented pressure-sealing packaging method can also be implemented in other microfluidic systems that require the sophisticated adjustment of ambient gas composition as well as the downstream experiment capacities. For instance, the same packaging method was used to incorporate different microfluidic pattern to study how bacterial population waves propagate through physical barriers22.
In summary, collective population dynamics are qualitatively different from single-&#173;cell behaviors. The microfluidic EA technology allows the quantitative study of the evolutionary dynamics and phenotypic behaviors individually and collectively as a function of time. This technology may present a more physiologically relevant in vitro model for cancer research, and potentially for preclinical drug development and screening.

Cancer has been increasingly recognized as a complex ecosystem that depends not only on the continued dysregulation of mutated cell populations but also on vital interactions between cancer cells and the host microenvironment. In this sense, cancer evolves on an adaptive landscape manifested by a combination of factors, including a heterogeneous tumor microenvironment and crosstalk with a variety of host cells, all of which contribute selective pressures for further genetic or epigenetic changes1,2,3. In the context of solid tumors, uneven distribution of chemotherapeutics and other resource gradients contributes to their molecular heterogeneity and may play a role in the development of drug resistance, increased angiogenesis to particular tumor subpopulations, and even metastasis4,5,6. Conventional in vitro 2D cell culture studies, while possessing large-scale, convenient experimental capacity, provides mean-field, uniform, and fixed conditions, often lacking the precise spatial and temporal environmental control necessary to truly emulate in vivo tumor dynamics. Thus, there is a need for more representative ex vivo models to reproduce the tumor microenvironment prior to animal models in the drug development pipeline in order for a better prediction of cancer progression as well as responses to drugs within dynamical stress landscapes. Microfluidics have been proposed to bridge the gap between 2D cell culture studies and more complex in vivo animal studies that may not be able to support controllable quantitative studies7,8,9.
An ideal in vitro system to characterize cancer cell dynamics should possess the ability to generate a heterogeneous microenvironment to mimic the adaptive cellular responses that may take place in a tumor, as well as allow for the observation of these dynamics at a single-cell resolution. In this article, we describe a microfluidic cell culture platform, a PDMS-based device called the &#34;Evolution Accelerator&#34; (EA), that allows for parallel in vitro studies of cancer cell dynamics at cellular resolution with real-time data acquisition over the course of weeks, while stably maintaining gradients of stress across the culture landscape. The design of this platform is based on our previous work, in which the evolutionary dynamics of organisms in a metapopulation can be accelerated10,11. Specifically, in a group of spatially separated populations that interact at some level, when exposed to a heterogeneous stress landscape, the most fit species can dominate in a local population faster compared with that of a large uniform population. The advantageous species then migrate to neighboring microhabitats in search of resources and space, and eventually dominate the entire population. As shown in Figure 1, the pattern of the microfluidic EA chip is composed of (i) a pair of serpentine channels that provide fresh media circulation and construct fixed boundary conditions for chemical diffusion, and (ii) the hexagonal cell culture region which consists 109 interconnected hexagonal and 24 half-hexagonal chambers in the center, resembling a honeycomb structure. The chip is 100 &#181;m in depth. Media channels and cell culture region are connected with small slits (about 15 &#181;m wide), which prevent direct media flow and the resulting shear stress across the cell culture area, yet still allow chemicals to diffuse through small slits and exchange nutrients, metabolic waste, etc. The generation of chemical gradients is demonstrated in Figure 1B, where one media channel contains 0.1 mM of fluorescein while the other channel is free of fluorescein. Cells are cultured on a gas permeable membrane, encapsulated by the microstructures through the positive back pressure on the membrane against the chip. The components of the device holder are illustrated in Figure 2, and the experimental setup is illustrated in Figure 3, where the culture is maintained on an inverted microscope at 37 &#176;C, with above 85% relative humidity, and conditioned under normoxia gas composition.
This system provides detailed observation of localized cellular interactions via brightfield and fluorescent channels and allows for spatially-resolved downstream assays such as immunofluorescence, Western blot, or mass spectrometry. We have previously demonstrated as a proof-of-principle of this microfluidic cancer-on-chip model on the long-term co-culture of epithelial and mesenchymal PC3 prostate cancer cells12 as well as the emergence of drug-resistance polyploid giant cancer cells using the epithelial PC3 cell line13. While we present the application of this platform to understand the spatiotemporal dynamics of epithelial PC3 and mesenchymal prostate cancer cells under a stress gradient of docetaxel, the microfluidic system can be easily applied to any combination of cell lines and resource (i.e., drug, nutrient, oxygen) gradients.

<table><tbody><tr><td>10 mL BD Luer-Lok tip syringes</td><td>BD</td><td>14-823-16E</td><td></td></tr><tr><td>Antibiotic-Antimycotic</td><td>Sigma-Aldrich</td><td>A5955</td><td>1x anti-anti</td></tr><tr><td>AZ 300 MIF</td><td>Merck KGaA</td><td>18441123163</td><td>Photoresist developer</td></tr><tr><td>AZ1518</td><td>Merck KGaA</td><td>AZ1518</td><td>Photoresist</td></tr><tr><td>AZ4330</td><td>Merck KGaA</td><td>AZ4330</td><td>Photoresist</td></tr><tr><td>Cr Chromium Etchant</td><td>Sigma-Aldrich</td><td>651826</td><td></td></tr><tr><td>Fetal bovine serum (FBS)</td><td>Life Technologies Corporation</td><td>10437028</td><td></td></tr><tr><td>Heidelberg DWL 66+ laserwriter</td><td>Heidelberg Instruments</td><td>DWL66+</td><td>Writing photomask</td></tr><tr><td>Hexamethyldisilazane (HMDS)</td><td>Sigma-Aldrich</td><td>379212</td><td>For photoresist adhesion enhancement</td></tr><tr><td>Hollow steel pins</td><td>New England Small Tube</td><td>NE-1300-01</td><td>&amp;nbsp;.025 OD .017 ID x .500 long / type 304 WD fullhard</td></tr><tr><td>ibidi Heating System, Multi-Well Plates, K-Frame</td><td>ibidi</td><td>10929</td><td>On-stage incubator&amp;nbsp;</td></tr><tr><td>Luer-Lok 23 G dispensing needle</td><td>McMaster-Carr</td><td>75165A684</td><td>To connect syringes and tubings</td></tr><tr><td>Lumox dish 35</td><td>Sarstedt</td><td>94.6077.331</td><td>Gas-permeable cell culture dish</td></tr><tr><td>Microposit Remover 1165</td><td>Dow Electronic Materials</td><td>Microposit Remover 1165</td><td>Photoresist stripper</td></tr><tr><td>Microseal B Adhesive Sealer</td><td>Bio-Rad Laboratories</td><td>MSB1001</td><td>Adhesive sealer</td></tr><tr><td>O-Ring (for Lumox plate sealing)</td><td>McMaster-Carr</td><td>9452K114</td><td>Dash No. 27; 1-5/16&quot; ID x 1-7/16&quot; OD; Duro 70</td></tr><tr><td>O-Ring (for bottom glass window sealing)</td><td>McMaster-Carr</td><td>9452K74</td><td>Dash No. 20; 7/8&quot; ID x 1&quot; OD; Duro 70</td></tr><tr><td>Plasma-Preen Plasma Cleaning/Etching System</td><td>Plasmatic Systems, Inc</td><td>Plasma-Preen</td><td>Oxygen plasma system</td></tr><tr><td>RPMI 1640</td><td>Life Technologies Corporation</td><td>11875-093</td><td></td></tr><tr><td>Samco RIE800iPB DRIE</td><td>Samco</td><td>RIE800iPB</td><td>Deep reactive-ion etching system</td></tr><tr><td>Suss MA6 mask aligner</td><td>SUSS MicroTec</td><td>MA6</td><td>Mask aligner&amp;nbsp;</td></tr><tr><td>Sylgard 184 Silicone Elastomer</td><td>Fisher Scientific</td><td>NC9285739</td><td>PDMS elastomer</td></tr><tr><td>TePla M4L plasma etcher</td><td>PVA TePla</td><td>M4L</td><td>Plasma etcher</td></tr><tr><td>Trichloro-1H,1H,2H,2H-perfluorooctyl-silane (PFOTS)</td><td>Sigma-Aldrich</td><td>448931</td><td>For silicon wafer silanization</td></tr><tr><td>Tygon microbore tube (0.020&quot; x 0.060&quot;OD)</td><td>Cole-Parmer</td><td>EW-06419-01</td><td>Tubings for media delivery</td></tr></tbody></table>

generation of heterogeneous drug gradients across cancer populations on a microfluidic evolution accelerator for real-time observation

Conventional cell culture remains the most frequently used preclinical model, despite its proven limited ability to predict clinical results in cancer. Microfluidic cancer-on-chip models have been proposed to bridge the gap between the oversimplified conventional 2D cultures and more complicated animal models, which have limited ability to produce reliable and reproducible quantitative results. Here, we present a microfluidic cancer-on-chip model that reproduces key components of a complex tumor microenvironment in a comprehensive manner, yet is simple enough to provide robust quantitative descriptions of cancer dynamics. This microfluidic cancer-on-chip model, the &#34;Evolution Accelerator,&#34; breaks down a large population of cancer cells into an interconnected array of tumor microenvironments while generating a heterogeneous chemotherapeutic stress landscape. The progression and the evolutionary dynamics of cancer in response to drug gradient can be monitored for weeks in real time, and numerous downstream experiments can be performed complementary to the time-lapse images taken through the course of the experiments.

Validation of optimum cell growth on chip 
A major goal of the experiment platform is to reproduce key components and interactions in a complex tumor microenvironment in a comprehensive manner, yet simple enough to provide quantitative, reliable and reproducible data. This goal can only be achieved if we have full control of the physical and biochemical environmental factors. We must either exclude the undesired factors or figure out a way to incorporate the uncontrollable factors into the quantitative model to correctly interpret the population behaviors.
The first test is to ensure optimum cell growth on the device. The cell proliferation rate on the device needs to be identical or comparable to their growth profile in conventional cell culture. As a proof of principle, human prostate cancer cell line PC3 cells were cultured in the PDMS chip without the presence of external stress. These cells were fluorescently-labeled in the cytoplasm so we could observe and quantify the population of cells using inverted fluorescent microscopy. Cells confluence, defined as the area that covered by cells, was measured at each microhabitat at different time frames given a selected intensity threshold on the fluorescent images using Fiji15. The growth curves of cells at each chosen position are plotted in Figure 4. The chosen positions are scattered across the chip, from the region near the apex of media inflow to the apex close to media outlets.
The growth curves in Figure 4B are well-aligned, suggesting the identicality of the cell proliferation profile as a function of position across the chip. The initial slope of the curves reveals the proliferation rate. The doubling time for cells in the device is around 24 hours as shown in Figure 4B from time 0 to 24 hours, which is the same as the doubling time in conventional cultureware13. Therefore, we conclude that without the presence of an external source of stress, the physical and biochemical factors are uniformly distributed, leading to the homogeneous and optimized cell growth from time 50 to 100 hours.
We further considered the ability to quantify cell dynamics between subpopulations in a microenvironment. GFP-expressing PC3-EMT and the mCherry-expressing PC3-EPI cell lines were co-cultured in the EA as shown in Figure 5. Cell confluence, defined as the percentage of area covered by the cells, is measured as the indication of the size of population. Starting from 40% confluence, the co-culture grew fully confluent within 3 days. Interestingly, we may observe the progression of each phenotype in the microenvironment. While the growth curve of total confluence is in the form of logistic growth model, the population of PC3-EMT continued to expand and PC3-EPI was suppressed in the asymptotic phase.
Demonstration of cell motility assay in a mixed population 
Cell motility is an important phenotypic behavior. The motility distribution of a population can provide information about the physical interaction of cells, the mechanical properties of local microenvironment, and can sometimes be analyzed as an indication of epigenetic variation of cells. Given that our improved cell culture platform allows nearly continuous imaging, the advantage of having fine temporal resolution maximizes the potential of single cell tracking in a heterogeneous population.
We use the plugin TrackMate16 in Fiji (http://fiji.sc) with customized macro to implement and automate the tracking process. TrackMate allows the user to implement and customize a tracking algorithm using a scripting language from the Fiji Script Editor. The tracking process is divided in a series of steps: the segmentation, filtering, and particle-linking processes.
As shown in Figure 6B, we performed a &#34;wound healing assay&#34; as a demonstration to study cell collective migration and cell-cell interaction. PC3-EPI and PC3-EMT cells were densely seeded in the center of the device and were allowed to freely migrate toward empty region. The normalized histogram of the speed of both phenotypes is plotted in Figure 6C. The velocity of PC3-EMT was significantly higher than PC3-EPI by a factor of 1.8x, which is consistent with the fact that the mesenchymal phenotype serves as a component of cutaneous wound healing with exceptional ability to migrate as opposed to the comparably stationary epithelial phenotype.
Further, in order to observe the progression of cell motility in a stress-free environment, we performed a long-term co-culture of PC3-EPI and PC3-EMT with uniform initial seeding density and tracked the distribution of cell velocity varying with time. As shown in Figure 7A,B, after 6 days of culture, as cells reached higher confluence, the distributions of cell speed for both phenotypes leaned toward the left tails.
We may compare the ratio of number of PC3-EPI to PC3-EMT in each class interval. As shown in Figure 7C, regardless of the days of culture or density of cells, PC3-EMT dominated the high-speed region while PC3-EPI occupied the low speed zone. Although the overall velocity decreased significantly for both phenotypes, PC3-EMT remained motile and was affected less by the crowdedness of the microenvironment as shown in Figure 7D. The average speed of PC3-EPI dropped around 40% while that of PC3-EMT only dropped 14%.
There are several factors that can affect the distribution of cell velocity and the average speed, such as the crowdedness of the population. Continuous cell tracking and monitoring over all subpopulation is essential to understand the progression of phenotypic behavior. For example, if we would like to quantify the level of the mesenchymal status of an unlabeled subpopulation, it would be more informative to acquire not only the distribution of the physical quantity (e.g., velocity) of the interested subpopulation as a function of time, but also that of all the rest of the coexisting subpopulation of cells.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/60185/60185fig1.jpg" /> 
Figure 1: The syringe-pump-driven microfluidic EA chip. (A) The microfluidic device has two separate medium inlets, two outlets, and one central port for cell seeding or extraction of excessive medium. Note that between the medium inlets and the cell culture arrays, a pair of serpentine channels that allow the medium to equilibrate with the atmosphere passed below the gas-permeable membrane. (B) The generation of gradient. The syringes pump the medium with ~ 0.1 mM of fluorescein and no fluorescein respectively into the chip through the 2 medium inlets on the right, extracted out from the chip at the 2 medium outlets on the left. The concentration of fluorescein is proportional to the intensity of fluorescence signal, and is profiled near the medium inlets/outlets a and near the center b. Figure reproduced with permission from Lin et al. 201712. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/60185/60185fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/60185/60185fig2.jpg" /> 
Figure 2: The components of the customized 3 well sample plate. (a) the main body of 3 well plate; (b) a pair of gas channels that allow conditioned atmosphere to be pumped in and vented out through the septa at the entrance of the gas channels; (c) an O-ring designed to seal the space between the well plate and the gas-permeable culture dish; (d) the 35 mm diameter gas-permeable culture dish; (e) the dish holder; (f) the PDMS device; (g) the PDMS chip holders; (h) the double layer 35 mm glass windows designed to maintain thermal isolation and prevent water condensation; (i) glass window holder; (j) heating pads; (k) temperature sensor; (l) the Adhesive sealer that keeps the chip from drying out. Figure reproduced with permission from Lin et al. 201712. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/60185/60185fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/60185/60185fig3.jpg" /> 
Figure 3: The schematic figure of the experimental setup. The setup of the experiment, including the gas supply system, gas channels connection, the medium supply connection and the imaging system. Figure reproduced with permission from Lin et al. 201712. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/60185/60185fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/60185/60185fig4.jpg" /> 
Figure 4: Growth curves of PC3 in the EA without stress. PC3 were cultured in EA without the presence of external stress. (A) Pattern of EA with position labels. (B) Growth curves of PC3 at the chosen positions in terms of cell confluence. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/60185/60185fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/60185/60185fig5.jpg" /> 
Figure 5: The co-culture of PC3-EPI and PC3-EMT in the EA without stress. PC3-EPI (red) and PC3-EMT (green) were co-cultured in the EA without the presence of external stress. (A) Overlay of two fluorescent channels at t = 0 h. (B) Fluorescent image taken at t = 95 h. (C) Growth curves in terms of cell confluence. Cell confluence of each cell type was measured on the entire chip. Each data point represents the average cell confluence at 3 consecutive time points taken at 15-min intervals. The error bars represent the standard deviation of cell confluence at the 3 consecutive time points. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/60185/60185fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/60185/60185fig6.jpg" /> 
Figure 6: Cell motility assay in a mixed population. The demonstration of single cell tracking performance in a mixed population. (A) A demonstration of how cells are detected by Laplacian of Gaussian (LoG) segmentation. The circles indicate the location of cells detected by the LoG algorithm. The detected cells are linked from frame to frame based on the linear assignment problem to quantify cell motility. (B) The &#34;wound healing assay&#34; of PC3-EPI and PC3-EMT co-culture experiment. Cells were seeded locally up to 100% confluence with a clear boundary at the center. After the installation of the EA chip, cells were observed to migrate through the microhabitat array as indicated by the white arrows. (C) Normalized histogram of cell motility. PC3-EMT is faster than PC3-EPI by a factor of 1.8x. The error bars represent the standard deviation of 5 experiment samples. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/60185/60185fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 7" class="xfigimg" src="/files/ftp_upload/60185/60185fig7.jpg" /> 
Figure 7: The motility assay of a long-term co-culture of PC3-EPI and PC3-EMT. A long-term co-culture of PC3-EPI and PC3-EMT with uniform initial seeding density. The distribution of cell velocity varies with time. (A) Normalized distribution of cell speed on day 2. (B) The normalized distribution of cell speed on day 6. (C) Ratio of number of PC3-EPI to PC3-EMT in each class interval. (D) Average speed of PC3-EPI and PC3-EMT as a function of time. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/60185/60185fig7large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Generation of Heterogeneous Drug Gradients Across Cancer Populations on a Microfluidic Evolution Accelerator for Real-Time Observation at JoVE.com

Generation of Heterogeneous Drug Gradients Across Cancer Populations on a Microfluidic Evolution Accelerator for Real-Time Observation

We present a microfluidic cancer-on-chip model, the &#34;Evolution Accelerator&#34; technology, which provides a controllable platform for long-term real-time quantitative studies of cancer dynamics within well-defined environmental conditions at the single-cell level. This technology is expected to work as an in vitro model for fundamental research or pre-clinical drug development.

Conventional cell culture remains the most frequently used preclinical model, despite its proven limited ability to predict clinical results in cancer. ...

generation-heterogeneous-drug-gradients-across-cancer-populations-on

Nanyang Technological University

Research

JoVE Journal

Bioengineering

6.3K Views.  Princeton University. Dit microfluïde kanker on-chip model dat we de evolutieversneller noemen, biedt een controleerbaar platform voor lange termijn, real-time kwantitatieve studies van kankerdynamica binnen goed gedefinieerde omgevingsomstandigheden op een enkelcellig niveau. De technologie stelt ons in staat om de evolutionaire dynamiek van kanker te onderzoeken onder een tumorachtig stresslandschap. Het verstrekken van informatie, waaronder morfologie, bevolking, beweeglijkheid, en migratie in de tijd op cellu...

Video: Generation of Heterogeneous Drug Gradients Across Cancer Populations on a Microfluidic Evolution Accelerator for Real-Time Observation

Microfluidic Device for Recreating a Tumor Microenvironment in Vitro

We have developed a microfluidic device that mimics the delivery and systemic clearance of drugs to heterogeneous three-dimensional tumor tissues in vitro. Nutrients delivered by vasculature fail to reach all parts of tumors, giving rise to heterogeneous microenvironments consisting of viable, quiescent and necrotic cell types. Many cancer drugs fail to effectively penetrate and treat all types of cells because of this heterogeneity. Monolayers of cancer cells do not mimic this heterogeneity, making it difficult to test cancer drugs with a suitable in vitro model. Our microfluidic devices were fabricated out of PDMS using soft lithography. Multicellular tumor spheroids, formed by the hanging drop method, were inserted and constrained into rectangular chambers on the device and maintained with continuous medium perfusion on one side. The rectangular shape of chambers on the device created linear gradients within tissue. Fluorescent stains were used to quantify the variability in apoptosis within tissue. Tumors on the device were treated with the fluorescent chemotherapeutic drug doxorubicin, time-lapse microscopy was used to monitor its diffusion into tissue, and the effective diffusion coefficient was estimated. The hanging drop method allowed quick formation of uniform spheroids from several cancer cell lines. The device enabled growth of spheroids for up to 3 days. Cells in proximity of flowing medium were minimally apoptotic and those far from the channel were more apoptotic, thereby accurately mimicking regions in tumors adjacent to blood vessels. The estimated value of the doxorubicin diffusion coefficient agreed with a previously reported value in human breast cancer. Because the penetration and retention of drugs in solid tumors affects their efficacy, we believe that this device is an important tool in understanding the behavior of drugs, and developing new cancer therapeutics.

Microfluidic Device for Recreating a Tumor Microenvironment in Vitro

We present the procedure for fabrication and operation of a microfluidic device that recreates heterogeneous tumor microenvironments in vitro. The variability in apoptosis within tumor tissue was quantified using fluorescent stains and the effective diffusion coefficient of the chemotherapeutic drug doxorubicin into tumor tissue was evaluated.

We have developed a microfluidic device that mimics the delivery and systemic clearance of drugs to heterogeneous three-dimensional tumor tissues in ...

A Gradient-generating Microfluidic Device for Cell Biology

 The fabrication and operation of a gradient-generating microfluidic device for studying cellular behavior is described.  A microfluidic platform is an enabling experimental tool, because it can precisely manipulate fluid flows, enable high-throughput experiments, and generate stable soluble concentration gradients.  Compared to conventional gradient generators, poly(dimethylsiloxane) (PDMS)-based  microfluidic devices can generate stable concentration gradients of growth factors with well-defined profiles.  Here, we developed simple gradient-generating microfluidic devices with three separate inlets.  Three microchannels combined into one microchannel to generate concentration gradients.  The stability and shape of growth factor gradients were confirmed by fluorescein isothyiocyanate (FITC)-dextran with a molecular weight similar to epidermal growth factor (EGF).  Using this microfluidic device, we demonstrated that fibroblasts exposed to concentration gradients of EGF migrated toward higher concentrations.  The directional orientation of cell migration and motility of migrating cells were quantitatively assessed by cell tracking analysis.  Thus, this gradient-generating microfluidic device might be useful for studying and analyzing the behavior of migrating cells.

We describe a protocol for the microfabrication of the gradient-generating microfluidic device that can generate spatial and temporal gradients in well-defined microenvironment. In this approach, the gradient-generating microfluidic device can be used to study directed cell migration, embryogenesis, wound healing, and cancer metastasis.

 The fabrication and operation of a gradient-generating microfluidic device for studying cellular behavior is described.  A microfluidic platform is an ...

Biology

Generation of High-Throughput Three-Dimensional Tumor Spheroids for Drug Screening

Cancer cells have routinely been cultured in two dimensions (2D) on a plastic surface. This technique, however, lacks the true environment a tumor mass is exposed to in vivo. Solid tumors grow not as a sheet attached to plastic, but instead as a collection of clonal cells in a three-dimensional (3D) space interacting with their neighbors, and with distinct spatial properties such as the disruption of normal cellular polarity. These interactions cause 3D-cultured cells to acquire morphological and cellular characteristics which are more relevant to in vivo tumors. Additionally, a tumor mass is in direct contact with other cell types such as stromal and immune cells, as well as the extracellular matrix from all other cell types. The matrix deposited is comprised of macromolecules such as collagen and fibronectin.
In an attempt to increase the translation of research findings in oncology from bench to bedside, many groups have started to investigate the use of 3D model systems in their drug development strategies. These systems are thought to be more physiologically relevant because they attempt to recapitulate the complex and heterogeneous environment of a tumor. These systems, however, can be quite complex, and, although amenable to growth in 96-well formats, and some now even in 384, they offer few choices for large-scale growth and screening. This observed gap has led to the development of the methods described here in detail to culture tumor spheroids in a high-throughput capacity in 1536-well plates. These methods represent a compromise to the highly complex matrix-based systems, which are difficult to screen, and conventional 2D assays. A variety of cancer cell lines harboring different genetic mutations are successfully screened, examining compound efficacy by using a curated library of compounds targeting the Mitogen-Activated Protein Kinase or MAPK pathway. The spheroid culture responses are then compared to the response of cells grown in 2D, and differential activities are reported. These methods provide a unique protocol for testing compound activity in a high-throughput 3D setting.

Across a wide variety of disease indications, more physiologically relevant models are being developed and implemented into drug discovery programs. The new model system described here demonstrates how three-dimensional tumor spheroids can be cultured and screened in a high-throughput 1536-well plate-based system to search for new oncology drugs.

Cancer cells have routinely been cultured in two dimensions (2D) on a plastic surface. This technique, however, lacks the true environment a tumor mass is ...

Cancer Research

Physiologic Patient Derived 3D Spheroids for Anti-neoplastic Drug Screening to Target Cancer Stem Cells

In this protocol, we outline the procedure for generation of tumor spheroids within 384-well hanging droplets to allow for high-throughput screening of anti-cancer therapeutics in a physiologically representative microenvironment. We outline the formation of patient derived cancer stem cell spheroids, as well as, the manipulation of these spheroids for thorough analysis following drug treatment. Specifically, we describe collection of spheroid morphology, proliferation, viability, drug toxicity, cell phenotype and cell localization data. This protocol focuses heavily on analysis techniques that are easily implemented using the 384-well hanging drop platform, making it ideal for high throughput drug screening. While we emphasize the importance of this model in ovarian cancer studies and cancer stem cell research, the 384-well platform is amenable to research of other cancer types and disease models, extending the utility of the platform to many fields. By improving the speed of personalized drug screening and the quality of screening results through easily implemented physiologically representative 3D cultures, this platform is predicted to aid in the development of new therapeutics and patient-specific treatment strategies, and thus have wide-reaching clinical impact.

This protocol describes generation of patient-derived spheroids, and downstream analysis including quantification of proliferation, cytotoxicity testing, flow cytometry, immunofluorescence staining and confocal imaging, in order to assess drug candidates&#8217; potential as anti-neoplastic therapeutics. This protocol supports precision medicine with identification of specific drugs for each patient and stage of disease.

In this protocol, we outline the procedure for generation of tumor spheroids within 384-well hanging droplets to allow for high-throughput screening of ...

Polydimethylsiloxane-polycarbonate Microfluidic Devices for Cell Migration Studies Under Perpendicular Chemical and Oxygen Gradients

This paper reports a microfluidic device made of polydimethylsiloxane (PDMS) with an embedded polycarbonate (PC) thin film to study cell migration under combinations of chemical and oxygen gradients. Both chemical and oxygen gradients can greatly affect cell migration in vivo; however, due to technical limitations, very little research has been performed to investigate their effects in vitro. The device developed in this research takes advantage of a series of serpentine-shaped channels to generate the desired chemical gradients and exploits a spatially confined chemical reaction method for oxygen gradient generation. The directions of the chemical and oxygen gradients are perpendicular to each other to enable straightforward migration result interpretation. In order to efficiently generate the oxygen gradients with minimal chemical consumption, the embedded PC thin film is utilized as a gas diffusion barrier. The developed microfluidic device can be actuated by syringe pumps and placed into a conventional cell incubator during cell migration experiments to allow for setup simplification and optimized cell culture conditions. In cell experiments, we used the device to study migrations of adenocarcinomic human alveolar basal epithelial cells, A549, under combinations of chemokine (stromal cell-derived factor, SDF-1&#945;) and oxygen gradients. The experimental results show that the device can stably generate perpendicular chemokine and oxygen gradients and is compatible with cells. The migration study results indicate that oxygen gradients may play an essential role in guiding cell migration, and cellular behavior under combinations of gradients cannot be predicted from those under single gradients. The device provides a powerful and practical tool for researchers to study interactions between chemical and oxygen gradients in cell culture, which can promote better cell migration studies in more in vivo-like microenvironments.

The control of chemical and oxygen gradients is essential for cell cultures. This paper reports a polydimethylsiloxane-polycarbonate (PDMS-PC) microfluidic device capable of reliably generating combinations of chemical and oxygen gradients for cell migration studies, which can be practically utilized in biological labs without sophisticated instrumentation.

This paper reports a microfluidic device made of polydimethylsiloxane (PDMS) with an embedded polycarbonate (PC) thin film to study cell migration under ...

An Organotypic High Throughput System for Characterization of Drug Sensitivity of Primary Multiple Myeloma Cells

In this work we describe a novel approach that combines ex vivo drug sensitivity assays and digital image analysis to estimate chemosensitivity and heterogeneity of patient-derived multiple myeloma (MM) cells. This approach consists in seeding primary MM cells freshly extracted from bone marrow aspirates into microfluidic chambers implemented in multi-well plates, each consisting of a reconstruction of the bone marrow microenvironment, including extracellular matrix (collagen or basement membrane matrix) and stroma (patient-derived mesenchymal stem cells) or human-derived endothelial cells (HUVECs). The chambers are drugged with different agents and concentrations, and are imaged sequentially for 96 hr through bright field microscopy, in a motorized microscope equipped with a digital camera. Digital image analysis software detects live and dead cells from presence or absence of membrane motion, and generates curves of change in viability as a function of drug concentration and exposure time. We use a computational model to determine the parameters of chemosensitivity of the tumor population to each drug, as well as the number of sub-populations present as a measure of tumor heterogeneity. These patient-tailored models can then be used to simulate therapeutic regimens and estimate clinical response.

We describe a high-throughput drug sensitivity assay for primary multiple myeloma cells. It consists of a reconstruction of the bone marrow microenvironment (including extracellular matrix and stroma) in multi-well plates, and a non-invasive method for longitudinal quantification of cell viability.

In this work we describe a novel approach that combines ex vivo drug sensitivity assays and digital image analysis to estimate chemosensitivity and ...

Medicine

3D Analysis of Multi-cellular Responses to Chemoattractant Gradients

Various limitations of 2D cell culture systems have sparked interest in 3D cell culture and analysis platforms, which would better mimic the spatial and chemical complexity of living tissues and mimic in vivo tissue functions. Recent advances in microfabrication technologies have facilitated the development of 3D in vitro environments in which cells can be integrated into a well-defined extracellular matrix (ECM) and a defined set of soluble or matrix associated biomolecules. However, technological barriers have limited their widespread use in research laboratories. Here, we describe a method to construct simple devices for 3D culture and experimentation with cells and multicellular organoids in 3D microenvironments with a defined chemoattractant gradient. We illustrate the use of this platform for analysis of the response of epithelial cells and organoids to gradients of growth factors, such as epidermal growth factor (EGF). EGF gradients were stable in the devices for several days leading to directed branch formation in breast organoids. This analysis allowed us to conclude that collective gradient sensing by groups of cells is more sensitive vs. single cells. We also describe the fabrication method, which does not require photolithography facilities nor advanced soft lithography techniques. This method will be helpful to study 3D cellular behaviors in the context of the analysis of development and pathological states, including cancer.

We describe a method to construct devices for 3D culture and experimentation with cells and multicellular organoids. This device allows analysis of cellular responses to soluble signals in 3D microenvironments with defined chemoattractant gradients. Organoids are better than single cells at detection of weak noisy inputs.

Various limitations of 2D cell culture systems have sparked interest in 3D cell culture and analysis platforms, which would better mimic the spatial and ...

Establishing Single-Cell Based Co-Cultures in a Deterministic Manner with a Microfluidic Chip

Cell co-culture assays have been widely used for studying cell-cell interactions between different cell types to better understand the biology of diseases including cancer. However, it is challenging to clarify the complex mechanism of intercellular interactions in highly heterogeneous cell populations using conventional co-culture systems because the heterogeneity of the cell subpopulation is obscured by the average values; the conventional co-culture systems can only be used to describe the population signal, but are incapable of tracking individual cells behavior. Furthermore, conventional single-cell experimental methods have low efficiency in cell manipulation because of the Poisson distribution. Microfabricated devices are an emerging technology for single-cell studies because they can accurately manipulate single cells at high-throughput and can reduce sample and reagent consumption. Here, we describe the concept and application of a microfluidic chip for multiple single-cell co-cultures. The chip can efficiently capture multiple types of single cells in a culture chamber (~46%) and has a sufficient culture space useful to study the cells&#39; behavior (e.g., migration, proliferation, etc.) under cell-cell interaction at the single-cell level. Lymphatic endothelial cells and oral squamous cell carcinoma were used to perform a single-cell co-culture experiment on the microfluidic platform for live multiple single-cell interaction studies.

This report describes a microfluidic chip-based method to set up a single cell culture experiment in which high-efficiency pairing and microscopic analysis of multiple single cells can be achieved.

Cell co-culture assays have been widely used for studying cell-cell interactions between different cell types to better understand the biology of diseases ...

Traction Microscopy Integrated with Microfluidics for Chemotactic Collective Migration

Cells change migration patterns in response to chemical stimuli, including the gradients of the stimuli. Cellular migration in the direction of a chemical gradient, known as chemotaxis, plays an important role in development, the immune response, wound healing, and cancer metastasis. While chemotaxis modulates the migration of single cells as well as collections of cells in vivo, in vitro research focuses on single-cell chemotaxis, partly due to the lack of the proper experimental tools. To fill that gap, described here is a unique experimental system that combines microfluidics and micropatterning to demonstrate the effects of chemical gradients on collective cell migration. Furthermore, traction microscopy and monolayer stress microscopy are incorporated into the system to characterize changes in cellular force on the substrate as well as between neighboring cells. As proof-of-concept, the migration of micropatterned circular islands of Madin-Darby canine kidney (MDCK) cells is tested under a gradient of hepatocyte growth factor (HGF), a known scattering factor. It is found that cells located near the higher concentration of HGF migrate faster than those on the opposite side within a cell island. Within the same island, cellular traction is similar on both sides, but intercellular stress is much lower on the side of higher HGF concentration. This novel experimental system can provide new opportunities to studying the mechanics of chemotactic migration by cellular collectives.

Collective cell migration in development, wound healing, and cancer metastasis is often guided by the gradients of growth factors or signaling molecules. Described here is an experimental system combining traction microscopy with a microfluidic system and a demonstration of how to quantify the mechanics of collective migration under biochemical gradient.

Cells change migration patterns in response to chemical stimuli, including the gradients of the stimuli. Cellular migration in the direction of a chemical ...

Generation of Dynamical Environmental Conditions using a High-Throughput Microfluidic Device

Mimicking in vivo environmental conditions is crucial for in vitro studies on complex life machinery. However, current techniques targeting live cells and organs are either highly expensive, like robotics, or lack nanoliter volume and millisecond time accuracy in liquid manipulation. We herein present the design and fabrication of a microfluidic system, which consists of 1,500 culture units, an array of enhanced peristaltic pumps and an on-site mixing modulus. To demonstrate the capacities of the microfluidic device, neural stem cell (NSC) spheres are maintained in the proposed system. We observed that when the NSC sphere is exposed to CXCL in day 1 and EGF in day 2, the round-shaped conformation is well maintained. Variation in the input order of 6 drugs causes morphological changes to the NSC sphere and the expression level representative marker for NSC stemness (i.e., Hes5 and Dcx). These results indicate that dynamic and complex environmental conditions have great effects on NSC differentiation and self-renewal, and the proposed microfluidic device is a suitable platform for high throughput studies on the complex life machinery.

We present a microfluidic system for high throughput studies on complex life machinery, which consists of 1500 culture units, an array of enhanced peristaltic pumps and an on-site mixing modulus. The microfluidic chip allows for the analysis of the highly complex and dynamic micro-environmental conditions in vivo.

Mimicking in vivo environmental conditions is crucial for in vitro studies on complex life machinery. However, current techniques targeting live cells and ...

Generation of Heterogeneous Drug Gradients Across Cancer Populations on a Microfluidic Evolution Accelerator for Real-Time Observation

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