This work was supported by the Ministry of Science and Technology of Taiwan under Grant Number 101-2221-E-002-064-MY3.

1. Fabrication of Microfluidic Device
<ol>
	<li>Use a graphic layout software (e.g., AutoCAD) to draw the outline of a T-microchannel. For the T-microchannel, the two feed channels are 90 &#181;m wide and 2,500 &#181;m long, and the confluence channel is 180 &#181;m wide and 3,000 &#181;m long. Connect the end of each channel to an individual circle with a diameter of 1,100 &#181;m.</li>
	<li>Mark &#8216;clear&#8217; and &#8216;dark&#8217; for the exposure and covered areas, respectively. For a negative photoresist (e.g., SU-8), the shape of the T-microchannel is &#8216;clear&#8217; and the surrounding is &#8216;dark.&#8217;</li>
	<li>Use a laser pattern generator with a wavelength of 442 nm and a minimum feature size of 2 &#956;m to transfer the pattern of the T-microchannel onto a chrome-on-glass photomask.</li>
	<li>Use the photomask, a substrate (e.g., single-side polished silicon wafer) and a permanent epoxy photoresist (e.g., SU-8) to make a mold through a standard lithography process. The photoresist layer is 55.2 &#956;m thick. In general, the photoresist thickness should be thinner than the depth of correlation of the objective lens17-19.</li>
	<li>Use the mold and a transparent material such as polydimethylsiloxane (PDMS) to fabricate the T-microchannel20.</li>
	<li>For fluidic connection, use a stainless steel tube of 2 mm in outer diameter to punch through-holes aligned to the circular patterns on the PDMS.</li>
	<li>Treat the surfaces of the PDMS and a glass slide with oxygen plasma at 60 W for 30 sec. Attach the PDMS to the glass slide. The oxidized surfaces of the two materials create a strong bond. Place the bonded PDMS structure on a hot plate for 5 min at 120 &#176;C.</li>
	<li>Insert Teflon tubes into the punched holes for fluidic connection.</li>
</ol>
2. Experimental Setup
<ol>
	<li>Construct the microscale schlieren system from a Hoffman modulation contrast microscope by removing the slit plate in the front focal plane of the condenser and replacing the modulator with a knife-edge in the rear focal plane of the 5X objective3. The depth of correlation, which depends on the numerical aperture of the objective17-19, should be sufficient to cover the entire depth of the microfluidic device. The surface of the knife-edge is blackened by anodic aluminum oxide to reduce its reflectivity.</li>
	<li>Mount the high-speed camera to the trinocular tube of the microscope via a C-mount adapter. Have the camera face the optical path of the microscope through a beam splitter. Connect the camera to a desktop computer via an Ethernet cable. Set the gamma correction to 1 for the camera so that its grayscale readout is proportional to the input luminance.</li>
	<li>Turn on the light source. In order to avoid excess heat, use LED (light emitting diode) lighting.</li>
	<li>Use an image processing software (e.g., function imread in MATLAB) to obtain the grayscale values of an acquired image. Remove the knife-edge, adjust the illumination, the aperture and the exposure time so that the average grayscale readout of the image is about 10% less than the maximal value. This denotes the background intensity for a 0% cutoff and we use a value of 230 for an 8-bit image.</li>
	<li>Insert the knife-edge to block the incident light completely. Record the average grayscale readout of the image. This denotes the background intensity for a 100% cutoff and the value is about 15 for an 8-bit image.</li>
	<li>Adjust the position of the knife-edge such that the average grayscale readout of the acquired image lies in the middle of the values for 0% and 100% cutoff. Now the degree of the cutoff is set to 50%.</li>
	<li>Prepare two transparent fluids with known refractive indices21 that are completely miscible with each other as the constituents. To evaluate the dependence of refractive index on concentration of the mixture, check the literature21 or use the Gladstone-Dale equation22. If the curve is nonlinear over the entire range, pick other fluid components. Then, choose a designated composition below which the refractive index of the solution varies linearly with the concentration. For example, use dilute aqueous ethanol with a mass fraction of 0.05 and water as the working fluids.</li>
	<li>Put the T-microchannel on the specimen stage. Arrange the T-microchannel so with the confluent channel parallel to the knife-edge (Figure 1).</li>
	<li>Prepare two identical syringes: syringe A is filled with the working fluid that serves as the reference fluid (water), and syringe B is filled with the other working fluid (dilute aqueous ethanol). The size of the syringe depends on the desired flow rate Q and the specification of the syringe pump: Q = &#960;d2V/4, where d is the inner diameter of the syringe and V is the speed of the plunger. Flow pulsation usually can be prevented by choosing a small syringe to increase V23.</li>
	<li>Collect the outlet fluid from the T-microchannel in a beaker. Ensure the Teflon outlet tube is fixed to the beaker&#39;s wall and its end is below the liquid level in the beaker in order to avoid vibration that would be caused by droplet breakoff.</li>
</ol>
3. Calibration
<ol>
	<li>Acquire the images of the two fluids mixing and the reference images.
	<ol>
		<li>At a given Reynolds number Re, set the flow rate of the syringe pumps, Q. Q is calculated from Q = &#181;(W+D)Re/4&#961;, where &#181; and &#961; are the viscosity and density of the working fluid, and W and D are the width and depth of the confluence channel of the T-microchannel, respectively.</li>
		<li>Load one pump with syringe A and the other pump with syringe B. Connect the two inlets of the T-microchannel to syringe A and syringe B via Teflon tubing. Start the syringe pumps to deliver the working fluids into the T-microchannel at identical volume flow rates.</li>
		<li>Wait until steady flow establishes. The steady flow condition is defined by the emergence of a stationary schlieren pattern.</li>
		<li>Use the camera controlled software to record twenty frames of fluidic mixing at a frame rate of 30 fps.</li>
		<li>Stop the pump which is loaded with syringe B. Only pump the reference fluid (water) through one inlet into the confluence channel of the T-microchannel at constant rate.</li>
		<li>Wait until steady flow condition is reached and no schlieren pattern is observed.</li>
		<li>Use the camera controlled software to take the reference image, when no optical inhomogeneity is present in the T-microchannel. Record twenty frames at a frame rate of 30 fps.</li>
		<li>Repeat 3.1.1 to 3.1.7 at different Reynolds number: Re = 1, 5, 10, 20 and 50 so that no complex flow structure emerges in the confluence region of the T-microchannel24.</li>
	</ol>
	</li>
	<li>Use an image processing software to divide the acquired image I(i, j) by the reference image I0(i, j)25, where i and j are the pixel indices.</li>
	<li>Employ a CFD (Computational Fluid Dynamics) package to simulate mixing of the designated fluids in the T-microchannel.
	<ol>
		<li>Construct the three-dimensional model for the geometry of the T-microchannel. Discretize the flow domain into structured grids. To increase the accuracy, employ finer mesh in the confluence and the central region of the T-microchannel.</li>
		<li>Assign the physical properties of fluids and establish the boundary conditions to the flow domain. During the solving process, determine the concentration-dependent diffusion coefficient from the concentration obtained in the last iteration26 in order to update the local concentration.</li>
		<li>Examine the sensitivities of the computed results by performing the grid study27.</li>
	</ol>
	</li>
	<li>For each node (xi, yi) on the xy-plane, employ the CFD post-processing tool to take the average values of the concentration field across the channel depth by the trapezoidal rule: w(xi, yj) = {&#8721;k [w(xi, yj, zk) + w(xi, yj, zk+1)]&#8729;(zk+1 - zk)/2}/D28, where D is the channel depth. Use the central differencing scheme to compute the derivative of concentration with respect to the cross-stream direction: (&#8706;w/&#8706;y)i, j = [w(xi, yj+1) - w(xi, yj-1)]/(yj+1 - yj-1).</li>
	<li>For both positive and negative gradients, extract the ratio of grayscale values I/I0 (obtained in 3.2) and the gradient of mass fraction &#8706;w/&#8706;y (obtained in 3.4) at specified locations such as y = 0 (centerline, streamwise direction) or various given x (cross-stream direction).</li>
	<li>Plot the results and determine the relationship between I/I0 and &#8706;w/&#8706;y, I/I0 = C1&#8706;w/&#8706;y + C2 (C1 and C2 are constants), with linear regression.</li>
</ol>
4. Quantitation
<ol>
	<li>Repeat steps 3.1 to 3.2 for mixing in the target microfluidic device. The depth of the target microfluidic device should be identical or close to that of the T-microchannel. If unsteady phenomenon is expected, acquire a video clip (sequence of images) in step 3.1.4 instead. The frame rate should be high enough to resolve the dynamics of the transient flow clearly, while the exposure time should be identical to the value used in 2.4, 2.5, 3.1.4 and 3.1.7.</li>
	<li>Use the relationship obtained in step 3.6 to convert the ratio of grayscale values to the gradient of mass fraction in the target microfluidic device.</li>
</ol>

<ol>
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The authors have nothing to disclose.

For fluidic mixing in a microfluidic device, the microscale schlieren technique is able to measure the magnitude of concentration gradient through quantifying change in light intensity. Because the principle of this technique relies on detecting the alternation of light propagation, the working fluids and the microfluidic device have to be transparent to the incident light. In addition, the protocol requires a linear relationship between the refractive index of the solution and its composition so that preliminary assessm...

Fluid mixing is an important issue that is found in many industrial processes and biological systems. With the emergence of microfluidics, mixing in microscale has brought much attention due to its challenge in diffusion domination among the mass transport mechanisms. Since designing an effective micromixer required quantitative validation, several measuring methods were developed5-7. Nevertheless, the three-dimensional structure, commonly found in efficient micromixers5, demands a more accurate representation of the concentration field that the common measuring techniques fail to deliver. Due to the limit of viewing angle8 or reaction kinetics6, the aforementioned methods may produce misleading results that do not correctly account for the homogeneity of the mixture.
For optically transparent fluids mixing in optically transparent microstructures, microscale schlieren technique3,9-14 provides an attractive alternative to analyze mixing inhomogeneity. In the past, microscale schlieren technique has been mostly used to visualize compressible flow9-13,15 or phase gradient16. Microscale schlieren technique benefits from both a simple optical layout and high sensitivity and enables not only the non-invasive investigation of specific flow feature that causes optical disturbance but is well suited for use in assessing mixing. In this paper, we construct the microscale schlieren system by inserting a knife-edge in the back focal plane of the objective of a microscope, describe a calibration procedure to realize quantitative analysis, and report a validation measurement in a microfluidic oscillator4. To implement measurements, the working fluids are properly selected so that the refractive index of the mixed fluids varies linearly with the composition, and the thickness of the target microfluidic device is identical to the one used in calibration. Besides species concentration, microscale schlieren technique can be extended to measure the gradient of other scalar quantity that is linearly correlated to the index of refraction, such as temperature or salinity.

<table border="0" cellpadding="0" cellspacing="0">
	<tbody>
		<tr>
			<td>Permanent Epoxy Negative Photoresist</td>
			<td>MicroChem</td>
			<td>SU-8 2150</td>
			<td></td>
		</tr>
		<tr>
			<td>single side polished silicon wafer</td>
			<td>Light Technology</td>
			<td>S4W1PP5SABUP1</td>
			<td>p-type, diameter: 100&#177;0.5 mm, thickness: 525 &#177;25 mm, orientation: (1 0 0)</td>
		</tr>
		<tr>
			<td>syringe pump</td>
			<td>kdScientific</td>
			<td>kds210</td>
			<td></td>
		</tr>
		<tr>
			<td>syringe, i.e. 10 ml</td>
			<td>Terumo</td>
			<td>SS-10L2138</td>
			<td></td>
		</tr>
		<tr>
			<td>Hoffman modulation contrast microscope</td>
			<td>Leica Microsystems</td>
			<td>DM IL LED</td>
			<td></td>
		</tr>
		<tr>
			<td>5X objective lens</td>
			<td>Leica Microsystems</td>
			<td>N PLAN</td>
			<td>NA = 0.12</td>
		</tr>
		<tr>
			<td>knife-edge</td>
			<td></td>
			<td></td>
			<td>custom made part</td>
		</tr>
		<tr>
			<td>camera, i.e. high speed</td>
			<td>Integrated Design Tools</td>
			<td>NX7-S1</td>
			<td></td>
		</tr>
		<tr>
			<td>C-mount adapter HC 0.63x</td>
			<td>Leica Microsystems</td>
			<td>541537</td>
			<td></td>
		</tr>
		<tr>
			<td>camera operating software</td>
			<td>Integrated Design Tools</td>
			<td>MotionPro X Studio 2.02.01</td>
			<td></td>
		</tr>
		<tr>
			<td>polydimethylsiloxane (PDMS)</td>
			<td>Dow Corning</td>
			<td>Sylgard-184 silicone elastomer kit</td>
			<td></td>
		</tr>
		<tr>
			<td>Teflon tubing, i.e. O.D. x I.D. 1/16 in. x 0.031 in.</td>
			<td>Supelco</td>
			<td>58700-U</td>
			<td></td>
		</tr>
		<tr>
			<td>micro glass slide</td>
			<td>Matsunami Glass</td>
			<td>S2215</td>
			<td></td>
		</tr>
		<tr>
			<td>hot plate</td>
			<td>Yeong-Shin</td>
			<td>HP-303DN</td>
			<td></td>
		</tr>
		<tr>
			<td>distilled water, i.e. HPLC grade</td>
			<td>Alps Chemicals</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>ethyl alcohol, i.e. reagent grade</td>
			<td>Nihon Shiyaku Reagent</td>
			<td>EA448652</td>
			<td></td>
		</tr>
		<tr>
			<td>image processing software</td>
			<td>Mathworks</td>
			<td>MATLAB R2009a</td>
			<td></td>
		</tr>
		<tr>
			<td>computational fluid dynamics package</td>
			<td>ESI group</td>
			<td>CFD-ACE+ 2008</td>
			<td></td>
		</tr>
	</tbody>
</table>

analyzing mixing inhomogeneity in a microfluidic device by microscale schlieren technique

In this paper, we introduce the use of microscale schlieren technique to measure mixing inhomogeneity in a microfluidic device. The microscale schlieren system is constructed from a Hoffman modulation contrast microscope, which provides easy access to the rear focal plane of the objective lens, by removing the slit plate and replacing the modulator with a knife-edge. The working principle of microscale schlieren technique relies on detecting light deflection caused by variation of refractive index1-3. The deflected light either escapes or is obstructed by the knife-edge to produce a bright or a dark band, respectively. If the refractive index of the mixture varies linearly with its composition, the local change in light intensity in the image plane is proportional to the concentration gradient normal to the optical axis. The micro-schlieren image gives a two-dimensional projection of the disturbed light produced by three-dimensional inhomogeneity.
To accomplish quantitative analysis, we describe a calibration procedure that mixes two fluids in a T-microchannel. We carry out a numerical simulation to obtain the concentration gradient in the T-microchannel that correlates closely with the corresponding micro-schlieren image. By comparison, a relationship between the grayscale readouts of the micro-schlieren image and the concentration gradients presented in a microfluidic device is established. Using this relationship, we are able to analyze the mixing inhomogeneity from associate micro-schlieren image and demonstrate the capability of microscale schlieren technique with measurements in a microfluidic oscillator4. For optically transparent fluids, microscale schlieren technique is an attractive diagnostic tool to provide instantaneous full-field information that retains the three-dimensional features of the mixing process.

The grayscale ratio I/I0 under different Reynolds number for both positive and negative gradients of mass fraction is shown (Figure 2) with a symmetrical band appearing in the middle of the T-microchannel. At low Reynolds number, the tail of the schlieren band is expanded and blurred due to the dispersion across the mixing interface. As the Reynolds number increases, the diffusion length shortens leading to a narrower band. At different downstream locations, the variations of...

Watch this Scientific Journal Video about Analyzing Mixing Inhomogeneity in a Microfluidic Device by Microscale Schlieren Technique at JoVE.com

Analyzing Mixing Inhomogeneity in a Microfluidic Device by Microscale Schlieren Technique

Herein, we describe a procedure that employs microscale schlieren technique to measure mixing inhomogeneity in a microfluidic device. Through calibration, distribution of concentration gradient can be derived from the micro-schlieren image.

In this paper, we introduce the use of microscale schlieren technique to measure mixing inhomogeneity in a microfluidic device. The microscale schlieren ...

analyzing-mixing-inhomogeneity-microfluidic-device-microscale

Research

JoVE Journal

Bioengineering

8.9K 조회수.  National Taiwan University. Herein, we describe a procedure that employs microscale schlieren technique to measure mixing inhomogeneity in a microfluidic device. Through calibration, distribution of concentration gradient can be derived from the micro-schlieren image. 

비디오: Analyzing Mixing Inhomogeneity in a Microfluidic Device by Microscale Schlieren Technique

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 Microfluidic Device for Studying Multiple Distinct Strains

The study of cell responses to environmental changes poses many experimental challenges: cells need to be imaged under changing conditions, often in a comparative manner. Multiwell plates are routinely used to compare many different strains or cell lines, but allow limited control over the environment dynamics. Microfluidic devices, on the other hand, allow exquisite dynamic control over the surrounding conditions, but it is challenging to image and distinguish more than a few strains in them. Here we describe a method to easily and rapidly manufacture a microfluidic device capable of applying dynamically changing conditions to multiple distinct yeast strains in one channel. The device is designed and manufactured by simple means without the need for soft lithography. It is composed of a Y-shaped flow channel attached to a second layer harboring microwells. The strains are placed in separate microwells, and imaged under the exact same dynamic conditions. We demonstrate the use of the device for measuring protein localization responses to pulses of nutrient changes in different yeast strains.

We present a simple method to produce microfluidic devices capable of applying similar dynamic conditions to multiple distinct strains, without the need for a clean room or soft lithography.

The study of cell responses to environmental changes poses many experimental challenges: cells need to be imaged under changing conditions, often in a ...

A Microfluidic Technique to Probe Cell Deformability

Here we detail the design, fabrication, and use of a microfluidic device to evaluate the deformability of a large number of individual cells in an efficient manner. Typically, data for ~102 cells can be acquired within a 1 hr experiment. An automated image analysis program enables efficient post-experiment analysis of image data, enabling processing to be complete within a few hours. Our device geometry is unique in that cells must deform through a series of micron-scale constrictions, thereby enabling the initial deformation and time-dependent relaxation of individual cells to be assayed. The applicability of this method to human promyelocytic leukemia (HL-60) cells is demonstrated. Driving cells to deform through micron-scale constrictions using pressure-driven flow, we observe that human promyelocytic (HL-60) cells momentarily occlude the first constriction for a median time of 9.3 msec before passaging more quickly through the subsequent constrictions with a median transit time of 4.0 msec per constriction. By contrast, all-trans retinoic acid-treated (neutrophil-type) HL-60 cells occlude the first constriction for only 4.3 msec before passaging through the subsequent constrictions with a median transit time of 3.3 msec. This method can provide insight into the viscoelastic nature of cells, and ultimately reveal the molecular origins of this behavior.

We demonstrate a microfluidics-based assay to measure the timescale for cells to transit through a sequence of micron-scale constrictions.

Here we detail the design, fabrication, and use of a microfluidic device to evaluate the deformability of a large number of individual cells in an ...

Protocol for Biofilm Streamer Formation in a Microfluidic Device with Micro-pillars

Several bacterial species possess the ability to attach to surfaces and colonize them in the form of thin films called biofilms. Biofilms that grow in porous media are relevant to several industrial and environmental processes such as wastewater treatment and CO2 sequestration. We used Pseudomonas fluorescens, a Gram-negative aerobic bacterium, to investigate biofilm formation in a microfluidic device that mimics porous media. The microfluidic device consists of an array of micro-posts, which were fabricated using soft-lithography. Subsequently, biofilm formation in these devices with flow was investigated and we demonstrate the formation of filamentous biofilms known as streamers in our device. The detailed protocols for fabrication and assembly of microfluidic device are provided here along with the bacterial culture protocols. Detailed procedures for experimentation with the microfluidic device are also presented along with representative results.

Protocols for the study of biofilm formation in a microfluidic device that mimics porous media are discussed. The microfluidic device consists of an array of micro-pillars and biofilm formation by Pseudomonas fluorescens in this device is investigated.

Several bacterial species possess the ability to attach to surfaces and colonize them in the form of thin films called biofilms. Biofilms that grow in ...

Layer-by-layer Collagen Deposition in Microfluidic Devices for Microtissue Stabilization

Although microfluidics provides exquisite control of the cellular microenvironment, culturing cells within microfluidic devices can be challenging. 3D culture of cells in collagen type I gels helps to stabilize cell morphology and function, which is necessary for creating microfluidic tissue models in microdevices. Translating traditional 3D culture techniques for tissue culture plates to microfluidic devices is often difficult because of the limited channel dimensions. In this method, we describe a technique for modifying native type I collagen to generate polycationic and polyanionic collagen solutions that can be used with layer-by-layer deposition to create ultrathin collagen assemblies on top of cells cultured in microfluidic devices. These thin collagen layers stabilize cell morphology and function, as shown using primary hepatocytes as an example cell, allowing for the long term culture of microtissues in microfluidic devices.

The creation of functional microtissues within microfluidic devices requires the stabilization of cell phenotypes by adapting traditional cell culture techniques to the limited spatial dimensions in microdevices. Modification of collagen allows the layer-by-layer deposition of ultrathin collagen assemblies that can stabilize primary cells, such as hepatocytes, as microfluidic tissue models.

Although microfluidics provides exquisite control of the cellular microenvironment, culturing cells within microfluidic devices can be challenging. 3D ...

Co-culture of Living Microbiome with Microengineered Human Intestinal Villi in a Gut-on-a-Chip Microfluidic Device

Here, we describe a protocol to perform long-term co-culture of multi-species human gut microbiome with microengineered intestinal villi in a human gut-on-a-chip microphysiological device. We recapitulate the intestinal lumen-capillary tissue interface in a microfluidic device, where physiological mechanical deformations and fluid shear flow are constantly applied to mimic peristalsis. In the lumen microchannel, human intestinal epithelial Caco-2 cells are cultured to form a &#39;germ-free&#39; villus epithelium and regenerate small intestinal villi. Pre-cultured microbial cells are inoculated into the lumen side to establish a host-microbe ecosystem. After microbial cells adhere to the apical surface of the villi, fluid flow and mechanical deformations are resumed to produce a steady-state microenvironment in which fresh culture medium is constantly supplied and unbound bacteria (as well as bacterial wastes) are continuously removed. After extended co-culture from days to weeks, multiple microcolonies are found to be randomly located between the villi, and both microbial and epithelial cells remain viable and functional for at least one week in culture. Our co-culture protocol can be adapted to provide a versatile platform for other host-microbiome ecosystems that can be found in various human organs, which may facilitate in vitro study of the role of human microbiome in orchestrating health and disease.

We describe an in vitro protocol to co-culture gut microbiome and intestinal villi for an extended period using a human gut-on-a-chip microphysiological system.

Here, we describe a protocol to perform long-term co-culture of multi-species human gut microbiome with microengineered intestinal villi in a human ...

Perfusable Vascular Network with a Tissue Model in a Microfluidic Device

A spheroid (a multicellular aggregate) is regarded as a good model of living tissues in the human body. Despite the significant advancement in the spheroid cultures, a perfusable vascular network in the spheroids remains a critical challenge for long-term culture required to maintain and develop their functions, such as protein expressions and morphogenesis. The protocol presents a novel method to integrate a perfusable vascular network within the spheroid in a microfluidic device. To induce a perfusable vascular network in the spheroid, angiogenic sprouts connected to microchannels were guided to the spheroid by utilizing angiogenic factors from human lung fibroblasts cultured in the spheroid. The angiogenic sprouts reached the spheroid, merged with the endothelial cells co-cultured in the spheroid, and formed a continuous vascular network. The vascular network could perfuse the interior of the spheroid without any leakage. The constructed vascular network may be further used as a route for supply of nutrients and removal of waste products, mimicking blood circulation in vivo. The method provides a new platform in spheroid culture toward better recapitulation of living tissues.

The protocol describes how to engineer a perfusable vascular network in a spheroid. The spheroid's surrounding microenvironment is devised to induce angiogenesis and connect the spheroid to the microchannels in a microfluidic device. The method allows the perfusion of the spheroid, which is a long-awaited technique in three-dimensional cultures.

A spheroid (a multicellular aggregate) is regarded as a good model of living tissues in the human body. Despite the significant advancement in the ...

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 ...

Formulating and Characterizing Lipid Nanoparticles for Gene Delivery using a Microfluidic Mixing Platform

Lipid-based drug carriers have been used for clinically and commercially available delivery systems due to their small size, biocompatibility, and high encapsulation efficiency. Use of lipid nanoparticles (LNPs) to encapsulate nucleic acids is advantageous to protect the RNA or DNA from degradation, while also promoting cellular uptake. LNPs often contain multiple lipid components including an ionizable lipid, helper lipid, cholesterol, and polyethylene glycol (PEG) conjugated lipid. LNPs can readily encapsulate nucleic acids due to the ionizable lipid presence, which at low pH is cationic and allows for complexation with negatively charged RNA or DNA. Here LNPs are formed by encapsulating messenger RNA (mRNA) or plasmid DNA (pDNA) using rapid mixing of the lipid components in an organic phase and the nucleic acid component in an aqueous phase. This mixing is performed using a precise microfluidic mixing platform, allowing for nanoparticle self-assembly while maintaining laminar flow. The hydrodynamic size and polydispersity are measured using dynamic light scattering (DLS). The effective surface charge on the LNP is determined by measuring the zeta potential. The encapsulation efficiency is characterized using a fluorescent dye to quantify entrapped nucleic acid. Representative results demonstrate the reproducibility of this method and the influence that different formulation and process parameters have on the developed LNPs.

Lipid nanoparticles are developed using a microfluidic mixing platform approach for mRNA and DNA encapsulation.

Lipid-based drug carriers have been used for clinically and commercially available delivery systems due to their small size, biocompatibility, and high ...

Preparation and Structural Evaluation of Epithelial Cell Monolayers in a Physiologically Sized Microfluidic Culture Device

In vitro microfluidic experimentation holds great potential to reveal many insights into the microphysiological phenomena occurring in conditions such as acute respiratory distress syndrome (ARDS) and ventilator-induced lung injury (VILI). However, studies in microfluidic channels with dimensions physiologically relevant to the terminal bronchioles of the human lung currently face several challenges, especially due to difficulties in establishing appropriate cell culture conditions, including media flow rates, within a given culture environment. The presented protocol describes an image-based approach to evaluate the structure of NCI-H441 human lung epithelial cells cultured in an oxygen-impermeable microfluidic channel with dimensions physiologically relevant to the terminal bronchioles of the human lung. Using phalloidin-based filamentous-actin staining, the cytoskeletal structures of the cells are revealed by confocal laser scanning microscopy, allowing for the visualization of individual as well as layered cells. Subsequent quantification determines whether the cell culture conditions being employed are producing uniform monolayers suitable for further experimentation. The protocol describes cell culture and layer evaluation methods in microfluidic channels and traditional fixed-well environments. This includes channel construction, cell culture and requisite conditions, fixation, permeabilization and staining, confocal microscopic imaging, image processing, and data analysis.

The presented protocol describes the development and use of a phalloidin-based filamentous-actin staining technique with confocal laser scanning microscopy (CLSM) to visualize adherent cell layer structure in microfluidic dynamic-culture channels and traditional fixed-well static-culture chambers. This approach aids in evaluating cell layer confluency, monolayer formation, and layer-thickness uniformity.

In vitro microfluidic experimentation holds great potential to reveal many insights into the microphysiological phenomena occurring in conditions such as ...