Name: preparation of primary acute lymphoblastic leukemia cells in different cell cycle phases by centrifugal elutriation
Uploaded: 2017-11-10T14:00:00.000+00:00
Duration: 9 min 9 s
Description: Watch this Scientific Journal Video about Preparation of Primary Acute Lymphoblastic Leukemia Cells in Different Cell Cycle Phases by Centrifugal Elutriation at JoVE.com

This work was supported by NIH CA109821 (to TCC). We thank Beckman-Coulter for generously providing funds to cover publication costs and for technical assistance in the set-up and operation of the elutriation system. We thank Dr. Fred Falkenburg for providing initial primary ALL cultures.

NOTE: This protocol has been optimized for primary B-ALL cells which range in diameter from approximately 8 &#181;m (G1 phase) to 13 &#181;m (G2/M phases). Thus, the specific centrifuge speeds and pump flow rates may not be applicable to cells with different size ranges. Nevertheless, appropriate elutriation parameters can be estimated using the sedimentation rate equation. Cells are cultured in a defined serum-free medium as described16 at an optimal density of 1 - 3 x 106 cells/mL. With the exception of the collection of fractions which is conducted at 4 &#176;C using ice-cooled tubes, all steps are conducted at room temperature and the centrifuge set at 20 &#176;C with a maximum of 24 &#176;C.
1. Preparation of Elutriation Buffer and Materials
<ol>
	<li>In order to reduce clumping of cells, prepare an elutriation buffer of Hank&#39;s balanced saline solution (HBSS) with phenol red supplemented with 2% fetal bovine serum (FBS), to protect cells from mechanical stress during the elutriation process, and 1.6 g/L of 2-naphthol-6,8-disulfonic acid dipotassium salt (NDA), which renders the cell exterior negatively charged and reduces clumping.
	<ol>
		<li>Add 1.6 g of NDA to a 50 mL conical tube.</li>
		<li>Under sterile conditions, add 35 mL of HBSS from a 1 L bottle to the 50 mL conical tube containing NDA. Swirl the tube until the NDA has dissolved.</li>
		<li>Using a 0.2 &#181;m filter, transfer the dissolved NDA into a new sterile 50 mL conical tube. Then add the NDA to the remaining 1 L of HBSS.</li>
		<li>Finally, add 21 mL FBS to the HBSS to obtain a final concentration of 2% (v/v). 
		NOTE: The elutriation buffer can be prepared and stored at 4 &#176;C until the expiration date on the HBSS or until there is a major change in the pH as indicated by a yellowing of the indicator dye.</li>
	</ol>
	</li>
	<li>Label 50 mL conical tubes for collection of fractions so that there are tubes labeled wash 1 and 2 (W1 and W2), fractions 1 - 20 (F1&#160;- F20), and STOP.
	<ol>
		<li>Pre-chill these tubes on ice before collecting fractions.</li>
	</ol>
	</li>
</ol>
2. Assembly of the Elutriation System
<ol>
	<li>First, install the strobe assembly into the centrifuge so that the power cord is fed out of the chamber through the port on the left side. Ensure that the strobe flash lamp is at the front of the chamber so it will line up with the viewing window when the centrifuge is closed.
	<ol>
		<li>Secure the assembly in place by first tightening two Phillips-head screws into the two holes at the top of the each bracket and then by tightening the thumbscrews at the bottom of each bracket.</li>
		<li>Plug the power cord into the strobe power port at the back of the centrifuge.</li>
	</ol>
	</li>
	<li>Next, set the rotor straight down onto the centrifuge drive hub and secure with a T-handle hex wrench. 
	NOTE: If the centrifuge is not needed for non-elutriation purposes, the strobe assembly and the rotor can be kept in the centrifuge between runs.</li>
	<li>Once the rotor is secured, place the quick-release assembly containing the elutriation chamber, counter balance, rotating seal assembly, and a mounting plate into the rotor.
	<ol>
		<li>Push down evenly with one hand on the elutriation chamber and the other hand on the counter balance until the bolts in the rotor snap into the holes on the mounting plate.</li>
		<li>Finally, attach the anchoring cable by placing the pin on one side of the cable into the hole in the rotating seal assembly and securing the eyehole on the other side of the cable with one of the Phillips-head screws (mentioned in 2.1.1) on the bracket on the left side of the chamber.</li>
	</ol>
	</li>
	<li>Next, assemble the flow system using a variable speed pump and tubing to pump buffer into the elutriation chamber and collect buffer as it flows out of the elutriation chamber.
	<ol>
		<li>Insert the size 16 input tubing coming from the variable speed pump through the port at the top left of the centrifuge chamber so that it enters into the chamber.</li>
		<li>Attach a fitting to the free end of the input tubing and insert the fitting into the input hole on the side of the rotating seal assembly.</li>
		<li>Insert the size 16 output tubing through the port and attach it to the transfer tube at the top of the rotating seal assembly. 
		NOTE: The flow system can also remain assembled between elutriation runs.</li>
	</ol>
	</li>
	<li>Lastly, turn the centrifuge on and set the specifications necessary for the experiment.
	<ol>
		<li>Change the rotor ID.</li>
		<li>If the centrifuge requires a time input, set for 2 h, which is more than sufficient to complete an elutriation run.</li>
		<li>Set the temperature to 20 &#176;C with a max temp of 24 &#176;C.</li>
		<li>Set the acceleration for max and the deceleration for slow.</li>
		<li>Finally, set the speed to 867 x g.</li>
	</ol>
	</li>
</ol>
3. Priming of the Elutriation System
<ol>
	<li>First in order to sterilize the elutriation system, place the reservoir tubing into a 500 mL plastic bottle containing 5% bleach and place the output tubing into an empty 1 L plastic waste bottle.
	<ol>
		<li>Turn the pump on and set the speed to 25 mL/min and allow the 5% bleach to flow all the way through the elutriation system until it is pumped out of the output tube into the waste bottle.</li>
		<li>Turn the centrifuge on and allow it to come to the maximum designated speed (867 x g) in order to release bubbles and backpressure.</li>
		<li>Stop the centrifuge. Once the rotor has stopped rotating, open the lid and inspect the chamber for any leaks.</li>
		<li>If there are no leaks, let the bleach solution flow through the system for at least 5 min.</li>
	</ol>
	</li>
	<li>Next, flush the system with autoclaved water as bleach can lead to formation of precipitates from the elutriation buffer which may lead to clumping of the cells, as well as cause harm to the cells.
	<ol>
		<li>Place the reservoir tubing into a 1 L bottle of autoclaved water and allow it to flush through for at least 10 min.</li>
	</ol>
	</li>
	<li>After flushing with water, introduce elutriation buffer into the system. Use a 150 mL glass bottle which has been autoclaved to create a reservoir for the elutriation buffer and cells.
	<ol>
		<li>Add 100 mL of elutriation buffer to the bottle and move the reservoir tubing to the glass bottle so that the tube is at the very bottom.</li>
		<li>Start the centrifuge and allow the buffer to flow through the system to flush out the water.</li>
		<li>Once the reservoir bottle is almost empty and the water is completely flushed out of the system, move the output tubing from the waste bottle to the reservoir so that the buffer is being recycled through the system.</li>
	</ol>
	</li>
	<li>Finally, adjust the viewing window so that the elutriation chamber can be seen at the current speed.
	<ol>
		<li>Press the strobe lamp power button on the outside of the centrifuge so that the lamp turns on. Turn the elutriation knob also on the outside of the centrifuge all the way to the left.</li>
		<li>While looking through the viewing window, slowly turn the knob to the right until the elutriation chamber comes into view and the strobe light is in time with the rotation of the rotor. 
		NOTE: The elutriation system can be left in this state until the cells are prepped.</li>
	</ol>
	</li>
</ol>
4. Preparation of the Cell Sample
<ol>
	<li>Count cells and aliquot 300 to 400 million in growth medium into several 50 mL conical tubes. Spin down the cells at 1210 x g for 3 min.</li>
	<li>Aspirate off growth media and resuspend cells in 25 mL of elutriation buffer by pipetting up and down gently.</li>
	<li>In order to reduce cell clumping, pass cells twice through a 25 gauge needle.
	<ol>
		<li>Using a 10 mL syringe draw up the cells and then attach 25 gauge needle and pass the cells through onto the inside wall of a sterile 50 mL conical tube. Repeat this until all 25 mL have passed through the needle.</li>
		<li>Obtain a new needle and syringe and repeat the process above once. 
		Caution: Syringe needles should be placed in sharps containers. 
		NOTE: It is critical that the cells are pushed through the needle immediately before introducing them to the elutriation system to keep cell clumping to a minimum.</li>
	</ol>
	</li>
</ol>
5. Introduction of Cell Sample into the Elutriation System and Collection of Fractions
<ol>
	<li>Introduce the cell sample into the elutriation system by pouring the cell sample into the reservoir tank which has the remaining elutriation buffer recycling through.
	<ol>
		<li>Let the cells enter into the system and reach equilibrium within the elutriation chamber. 
		NOTE: This process will take about 5 min and progress can be tracked by watching the cells as they enter the chamber via the viewing window. To ensure all cells are in the chamber, take a drop of eluent, place on a glass slide, and view under a microscope. If the sample is free of intact cells, this confirms their retention in the chamber.</li>
	</ol>
	</li>
	<li>Start collecting fractions once all the cells have entered into the chamber and there is a distinct boundary at the widest part of the chamber in which the cells are in equilibrium.
	<ol>
		<li>Begin by moving the output tube to the 50 mL conical tube labeled W1. Collect 50 mL of elutriation buffer for this fraction, making sure to keep an eye on the reservoir tank and replenish with elutriation buffer when necessary. 
		NOTE: In order to make sure that all cells have entered into the system, allow the reservoir tank to become almost empty before refilling the reservoir the first time. After the first refill it will not be necessary to wait for the reservoir to become almost empty. Also, DO NOT ever allow the tank to become empty as this will create bubbles and back pressure in the system.</li>
		<li>Once 50 mL have been collected for W1, simultaneously change the speed to 821 x g and move the output tube to the conical tube labeled W2 and collect 50 mL more at this speed.</li>
		<li>Continue changing the speed and collecting fractions as indicated in Table 1. Make sure there is media in the reservoir tank and keep the conical tubes on ice at all times. Finally, adjust the viewing window by slowly turning the knob to the right as the speed decreases.</li>
		<li>Once all 20 fractions have been collected, stop the centrifuge and collect 50 mL in the conical tube labeled STOP.</li>
	</ol>
	</li>
</ol>
6. Flushing of the Elutriation System
<ol>
	<li>After the centrifuge has stopped completely flush the system by putting the reservoir tube in the 1 L bottle of autoclaved water and the output tube back in the waste bottle.
	<ol>
		<li>Turn the pump speed up to 50 mL/min and allow the water to run through the system until it is depleted.</li>
	</ol>
	</li>
	<li>Turn off the pump, remove the input and output hose from the quick-release assembly, and pull out the pin from the anchoring cable.
	<ol>
		<li>Remove the quick-release assembly from the rotor. 
		NOTE: Depending on what the centrifuge will be used for, the elutriation system can now be left as is. Otherwise, the whole assembly can be taken down in the opposite order as described above.The elutriation chamber can be removed from the quick-release assembly and cleaned between runs using an ultrasonic water bath. This removes debris and contaminants from the chamber wall which may negatively affect later runs.</li>
	</ol>
	</li>
</ol>
7. Analysis of Fractions and Collection of the G1 or G2/M Pools.
Note: In order to demonstrate the effectiveness of elutriation, each fraction is analyzed for cell count, cell diameter, and DNA content, and pools are created of cells in the G1 or G2/M phases for immunoblot analyses, as described in Representative Results. This protocol section will describe how to create these pools and prepare them for experimental use.
<ol>
	<li>Spin each fraction at 2000 x g for 5 min at 4 &#176;C and aspirate off elutriation buffer.</li>
	<li>Combine fractions together in order to obtain both a G1 phase pool and a G2/M phases pool.
	<ol>
		<li>For the G1 phase pool, resuspend fractions which were collected in the speed range of 788 x g to 661 x g (F1 - F5) in a total 1 mL of phosphate buffer saline solution (PBS) and transfer to a 15 mL conical tube. For the G2/M phases pool, resuspend fractions which were collected in the speed range of 387 x g and 333 x g (F17 - F20).</li>
		<li>Spin down cells at 2000 x g for 5 min at 4 &#176;C and aspirate off PBS.</li>
	</ol>
	</li>
	<li>Resuspend cells in 10 mL of growth media and take a cell count.</li>
	<li>Take an aliquot from each pool to be analyzed for DNA content via propidium iodide staining and flow cytometric analysis15. 
	NOTE: The remainder of each pool can be used for further experiments.</li>
</ol>

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Anisha Kothari is currently at&#160;the Department of Cell and Molecular Biology at St. Jude Children&#39;s Research Hospital.

We have described a method for obtaining primary ALL cells in different phases of the cell cycle using CCE. Under optimal conditions an essentially pure population of cells in G1 phase and a highly enriched population of cells in G2/M phases could readily be obtained in excellent yield, and cells highly enriched in S phase can also be obtained if desired. The results presented here were obtained using one primary ALL culture (specifically, ALL-5), and essentially identical results have been obtained with an independent c...

Cultured cells typically grow asynchronously and individual cells are present in different phases of the cell cycle. Some organisms exhibit naturally synchronous cell cycles or can be synchronized by specific physiological stimuli. For example, nuclei within giant plasmodia of the slime mold Physarum polycephalum divide in a highly synchronous fashion1, and cells of the green algae Desmodesmus quadricauda can be synchronized by alternating light and dark periods2. While such organisms offer unique experimental attributes, they inadequately model the complexities of mammalian cells. The ability to artificially synchronize mammalian cell populations has been central to advancing our understanding of cell cycle regulation and the molecular basis of cell cycle checkpoints. Common methods include serum deprivation, chemical block and release, or exploiting physical characteristics3,4. Withdrawal of serum often causes cells to enter quiescence, and the re-addition of serum promotes cell cycle reentry into the G1 phase5. Chemical inhibitors include agents such as excess thymidine or hydroxyurea which block cells at the G1/S boundary, or microtubule inhibitors which typically arrest cells in the M phase3,4. Approaches that exploit physical characteristics include mitotic shake-off which can be used to enrich for mitotic cells since they are less adherent than interphase cells6. However, all of these techniques have potential drawbacks. For example, not all cell types maintain viability in the absence of serum or the presence of chemical inhibitors, and the yield of cells after mitotic shake-off is limited without prior synchronization with mitotic inhibitors.
With the exception of early embryonic cell cycles, where cells progressively decrease in size as they divide7, most cells advancing through the cycle undergo growth phases and become larger. This property is exploited in the technique of counterflow centrifugal elutriation (CCE), which can be used to separate cells differing in size and hence in cell cycle phase8,9. During CCE, cells are under the influence of two opposing forces: centrifugal force, which drives the cells away from the axis of rotation, and fluid velocity (counterflow), which drives the cells towards the axis of rotation (Figure 1). Cells in the elutriation chamber reach an equilibrium position where these forces are equal. The key factors dictating the equilibrium position are cell diameter and density. As the flow rate of the buffer solution is increased and the counterflow drag force outweighs the centrifugal force, a new equilibrium is established, causing a change in position of cells inside the chamber. All cells are shifted toward the chamber exit, resulting in smaller ones leaving the chamber first, whereas the larger cells stay within the chamber until the counterflow rate is increased sufficiently to promote their exit. The cells escaping the elutriation chamber with consecutive increases in counterflow rate can be collected in specific fractions and each fraction contains cells of sequentially increasing sizes. Instead of conducting elutriation with incremental increases in counterflow rate, sequential decreases in centrifugal force by decreasing centrifugation speed will accomplish the same result. The process of elutriation requires optimization depending on cell type, elutriation buffer employed, and the specific apparatus used. The rate of sedimentation of cells under these conditions is best described by Stokes Law: SV = [d2(&#961;p-&#961;m)/18&#951;].&#969;2r, where SV = sedimentation velocity; d = diameter of the particle; &#961;p = density of the particle; &#961;m = density of the buffer; &#951; = viscosity of the buffer; &#969; = angular velocity of the rotor; and r = radial position of the particle. Thus, SV is proportional to cell diameter and density, and since diameter is raised to the second power, it contributes more significantly than density which is generally constant through the cell cycle.
An important advantage of CCE is that cells are not subjected to harsh conditions of chemical treatment or nutritional deprivation and can be recovered in excellent yield essentially unperturbed. A requirement is that the cells in question undergo a significant increase in diameter, of at least 30%, as they traverse the cell cycle. The main disadvantage is the cost of the specialized centrifuge, rotor, and accessories. Nonetheless, the ability to prepare cells enriched in specific cell cycle phases by CCE has greatly facilitated cell cycle research in organisms from yeast to mammalian cells9,10. Moreover, recent advances are expanding uses to the separation of cells from healthy versus cancerous tissue, the separation of different cell types in heterogeneous mixtures, and to the production of specific cell types for immunotherapy9.
Our major interest has been in understanding the mechanism of action of microtubule targeting agents (MTAs) such as vinca alkaloids and taxanes. These drugs were thought to act exclusively in mitosis, blocking spindle microtubule function11,12, but recent evidence suggests they may also target interphase microtubules13,14. We recently reported that primary acute lymphoblastic leukemia (ALL) cells undergo death in either the G1 phase or in the M phase when treated with vincristine and other MTAs in a cell cycle-dependent manner15. The ability to separate ALL cells into different cell cycle phases by CCE was instrumental in reaching this conclusion. In this article, we describe the technical details and offer practical tips for the application of CCE to the preparation of primary ALL cells in different cell cycle phases.

<table><tbody><tr><td>Hanks&#039; balanced salt solution</td><td>Lonza</td><td>10-508Q</td><td>1 L bottle</td></tr><tr><td>Fetal Plus bovine serum</td><td>Atlas Biologicals</td><td>FP-0500-A</td><td>500 mL bottle</td></tr><tr><td>2-napthol-6,8-disulfonic acid dipotassium salt</td><td>Acros Organics</td><td>212-672-4</td><td>100 g powder</td></tr><tr><td>50 mL concial tubes</td><td>Denville Scientifics</td><td>C1062-P</td><td>500/case</td></tr><tr><td>PES Membrane 0.22 &amp;micro;m filter unit</td><td>Millipore</td><td>SLGP033RB</td><td>250/pack</td></tr><tr><td>Avanti J-26S XPI w/ Elut. Non-IVD - 50/60 Hz, 200/208/240V</td><td>Beckman Coulter</td><td>B14544</td><td>centrifuge compatible with elutriation system</td></tr><tr><td>JE 5.0 elutriator rotor kit</td><td>Beckman Coulter</td><td>356900</td><td>rotor kit which includes the rotor, T-handle hex wrench, the quick release assembly (w/o the elutriation chamber), anchoring cable, and the strobe assembly</td></tr><tr><td>Chamber, standard, 4-mL, &quot;A&quot;</td><td>Beckman Coulter</td><td>356943</td><td>standard elutriation chamber&amp;nbsp;</td></tr><tr><td>Masterflex L/S Easy-Load pump head</td><td>Cole-Parmer</td><td>EW-07518-10</td><td></td></tr><tr><td>Masterflex L/S Variable-Speed Drive</td><td>Cole-Parmer</td><td>EW-07528-10</td><td></td></tr><tr><td>Masterflex BioPharm platinum-cured silicone pump tubing, L/S 16</td><td>Cole-Parmer</td><td>EW-96420-16</td><td></td></tr><tr><td>25 G x 1.5 Precision Glide needle</td><td>BD</td><td>305127</td><td>sterile, single-use needles</td></tr><tr><td>10 mL Luer-Lok syringe</td><td>BD</td><td>309604</td><td>sterile, single-use syringes</td></tr><tr><td>Vi-Cell XR</td><td>Beckman Coulter</td><td>383556</td><td></td></tr><tr><td>PI/RNase staining buffer</td><td>BD Pharmingen</td><td>550825</td><td>propidium iodide/RNase staining buffer</td></tr><tr><td>cyclin B1 (GNS1) mouse monoclonal IgG antibody</td><td>Santa Cruz Biotechnology</td><td>sc-245</td><td></td></tr><tr><td>cyclin D1 (DCS-6) mouse monoclonal IgG antibody</td><td>Santa Cruz Biotechnology</td><td>sc-20044</td><td></td></tr><tr><td>P-Rb (S807/811) (D20B12) XPR rabbit monoclonal antibody</td><td>Cell Signaling Technology</td><td>8516s</td><td></td></tr><tr><td>GAPDH (14C10) rabbit monoclonal antibody</td><td>Cell Signaling Technology</td><td>2118s</td><td></td></tr><tr><td>Goat anti-mouse IgG (H+L)-HRP conjugate</td><td>BioRad</td><td>170-6516</td><td></td></tr><tr><td>Goat anti-rabbit IgG (H+L)-HRP conjugate</td><td>BioRad</td><td>170-6515</td><td></td></tr></tbody></table>

preparation of primary acute lymphoblastic leukemia cells in different cell cycle phases by centrifugal elutriation

The ability to synchronize cells has been central to advancing our understanding of cell cycle regulation. Common techniques employed include serum deprivation; chemicals which arrest cells at different cell cycle phases; or the use of mitotic shake-off which exploits their reduced adherence. However, all of these have disadvantages. For example, serum starvation works well for normal cells but less well for tumor cells with compromised cell cycle checkpoints due to oncogene activation or tumor suppressor loss. Similarly, chemically-treated cell populations can harbor drug-induced damage and show stress-related alterations. A technique which circumvents these problems is counterflow centrifugal elutriation (CCE), where cells are subjected to two opposing forces, centrifugal force and fluid velocity, which results in the separation of cells on the basis of size and density. Since cells advancing through the cycle typically enlarge, CCE can be used to separate cells into different cell cycle phases. Here we apply this technique to primary acute lymphoblastic leukemia cells. Under optimal conditions, an essentially pure population of cells in G1 phase and a highly enriched population of cells in G2/M phases can be obtained in excellent yield. These cell populations are ideally suited for studying cell cycle-dependent mechanisms of action of anticancer drugs and for other applications. We also show how modifications to the standard procedure can result in suboptimal performance and discuss the limitations of the technique. The detailed methodology presented should facilitate application and exploration of the technique to other types of cells.

Primary ALL cells (3 - 4 x 108) were subjected to centrifugal elutriation and collected into two wash fractions and twenty main fractions, as described in the protocol. Table 1 shows representative data where the total number of cells in each fraction as well as the corresponding rotor speed are presented. Overall yield was typically over 80%. Measurement of cell diameter in individual fractions confirmed that cell diameter increased with advancing elutriation (<strong class="x...

Watch this Scientific Journal Video about Preparation of Primary Acute Lymphoblastic Leukemia Cells in Different Cell Cycle Phases by Centrifugal Elutriation at JoVE.com

Preparation of Primary Acute Lymphoblastic Leukemia Cells in Different Cell Cycle Phases by Centrifugal Elutriation

This protocol describes the use of centrifugal elutriation to separate primary acute lymphoblastic leukemia cells into different cell cycle phases.

The ability to synchronize cells has been central to advancing our understanding of cell cycle regulation. Common techniques employed include serum ...

preparation-primary-acute-lymphoblastic-leukemia-cells-different-cell

Universidad San Sebastian

Research

JoVE Journal

Cancer Research

8.2K Views.  University of Arkansas for Medical Sciences. This protocol describes the use of centrifugal elutriation to separate primary acute lymphoblastic leukemia cells into different cell cycle phases. 

Video: Preparation of Primary Acute Lymphoblastic Leukemia Cells in Different Cell Cycle Phases by Centrifugal Elutriation

A Chromatin Immunoprecipitation Assay to Identify Novel NFAT2 Target Genes in Chronic Lymphocytic Leukemia

Chronic lymphocytic leukemia (CLL) is characterized by the expansion of malignant B cell clones and represents the most common leukemia in western countries. The majority of CLL patients show an indolent course of the disease as well as an anergic phenotype of their leukemia cells, referring to a B cell receptor unresponsive to external stimulation. We have recently shown that the transcription factor NFAT2 is a crucial regulator of anergy in CLL. A major challenge in the analysis of the role of a transcription factor in different diseases is the identification of its specific target genes. This is of&#160;great significance for the elucidation of pathogenetic mechanisms and potential therapeutic interventions. Chromatin immunoprecipitation (ChIP) is a classic technique to demonstrate protein-DNA interactions and can, therefore, be used to identify direct target genes of transcription factors in mammalian cells. Here, ChIP was used to identify LCK as a direct target gene of NFAT2 in human CLL cells. DNA and associated proteins are crosslinked using formaldehyde and subsequently sheared by sonication into DNA fragments of approximately 200-500 base pairs (bp). Cross-linked DNA fragments associated with NFAT2 are then selectively immunoprecipitated from cell debris using an &#945;NFAT2 antibody. After purification, associated DNA fragments are detected via quantitative real-time PCR (qRT-PCR). DNA sequences with evident enrichment represent regions of the genome which are targeted by NFAT2 in vivo. Appropriate shearing of the DNA and the selection of the required antibody are particularly crucial for the successful application of this method. This protocol is ideal for the demonstration of direct interactions of NFAT2 with target genes. Its major limitation is the difficulty to employ ChIP in large-scale assays analyzing the target genes of multiple transcription factors in intact organisms.

Chronic lymphocytic leukemia (CLL) is the most common leukemia in the western world. NFAT transcription factors are important regulators of development and activation in numerous cell types. Here, we present a protocol for the use of chromatin immunoprecipitation (ChIP) in human CLL cells to identify novel target genes of NFAT2.

Chronic lymphocytic leukemia (CLL) is characterized by the expansion of malignant B cell clones and represents the most common leukemia in western ...

Subcellular Fractionation of Primary Chronic Lymphocytic Leukemia Cells to Monitor Nuclear/Cytoplasmic Protein Trafficking

Nuclear export of macromolecules is often deregulated in cancer cells. Tumor suppressor proteins, such as p53, can be rendered inactive due to aberrant cellular localization disrupting their mechanism of action. The survival of chronic lymphocytic leukaemia (CLL) cells, among other cancer cells, is assisted by the deregulation of nuclear to cytoplasmic shuttling, at least in part through deregulation of the transport receptor XPO1 and the constitutive activation of PI3K-mediated signaling pathways. It is essential to understand the role of individual proteins in the context of their intracellular location to gain a deeper understanding of the role of such proteins in the pathobiology of the disease. Furthermore, identifying processes that underlie cell stimulation and the mechanism of action of specific pharmacological inhibitors, in the context of subcellular protein trafficking, will provide a more comprehensive understanding of the mechanism of action. The protocol described here enables the optimization and subsequent efficient generation of nuclear and cytoplasmic fractions from primary chronic lymphocytic leukemia cells. These fractions can be used to determine changes in protein trafficking between the nuclear and cytoplasmic fractions upon cell stimulation and drug treatment. The data can be quantified and presented in parallel with immunofluorescent images, thus providing robust and quantifiable data.

This protocol enables the optimization and subsequent efficient generation of nuclear and cytoplasmic fractions from primary chronic lymphocytic leukemia cells. These samples are used to determine protein localization as well as changes in protein trafficking that take place between the nuclear and cytoplasmic compartments upon cell stimulation and drug treatment.

Nuclear export of macromolecules is often deregulated in cancer cells. Tumor suppressor proteins, such as p53, can be rendered inactive due to aberrant ...

From a 2DE-Gel Spot to Protein Function: Lesson Learned From HS1 in Chronic Lymphocytic Leukemia

The identification of molecules involved in tumor initiation and progression is fundamental for understanding disease&#8217;s biology and, as a consequence, for the clinical management of patients. In the present work we will describe an optimized proteomic approach for the identification of molecules involved in the progression of Chronic Lymphocytic Leukemia (CLL). In detail, leukemic cell lysates are resolved by 2-dimensional Electrophoresis (2DE) and visualized as &#8220;spots&#8221; on the 2DE gels. Comparative analysis of proteomic maps allows the identification of differentially expressed proteins (in terms of abundance and post-translational modifications) that are picked, isolated and identified by Mass Spectrometry (MS). The biological function of the identified candidates can be tested by different assays (i.e. migration, adhesion and F-actin polymerization), that we have optimized for primary leukemic cells.

Here we describe a protocol that couples two proteomic techniques, namely 2-dimensional Electrophoresis (2DE) and Mass Spectrometry (MS), to identify differentially expressed/post-translational modified proteins among two or more groups of primary samples. This approach, together with functional experiments, allows the identification and characterization of prognostic markers/therapeutic targets.

The identification of molecules involved in tumor initiation and progression is fundamental for understanding disease&#8217;s biology and, as a ...

Medicine

A Simple Red Blood Cell Lysis Method for the Establishment of B Lymphoblastoid Cell Lines

A number of methods exist for the transformation of B lymphocytes by the Epstein Barr virus in vitro into immortalized cell lines. We have developed a new method with a powerful and simple strategy for the establishment of B-LCLs, the red blood cell lysis method. This method simplified the PBMC separation procedure with red blood cell removal, and used as little as 0.5 mL of whole blood for establishing EBV-immortalized cell lines, which can proliferate to large cell numbers in a relatively short amount time with a 100% success rate. The method is simple, reliable, time saving, and applicable to treating a large number of the clinical samples.

A simple red blood cell lysis method for establishing B-LCLs was developed with high immortalization efficiency, requiring a small amount of blood and saving time from initiation to cryopreservation.

A number of methods exist for the transformation of B lymphocytes by the Epstein Barr virus in vitro into immortalized cell lines. We have developed a new ...

Immunology and Infection

Modeling Chemotherapy Resistant Leukemia In Vitro

It is well established that the bone marrow microenvironment provides a unique site of sanctuary for hematopoietic diseases that both initiate and progress in this site. The model presented in the current report utilizes human primary bone marrow stromal cells and osteoblasts as two representative cell types from the marrow niche that influence tumor cell phenotype. The in vitro co-culture conditions described for human leukemic cells with these primary niche components support the generation of a chemoresistant subpopulation of tumor cells that can be efficiently recovered from culture for analysis by diverse techniques. A strict feeding schedule to prevent nutrient fluxes followed by gel type 10 cross-linked dextran (G10) particles recovery of the population of tumor cells that have migrated beneath the adherent bone marrow stromal cells (BMSC) or osteoblasts (OB) generating a "phase dim" (PD) population of tumor cells, provides a consistent source of purified therapy resistant leukemic cells. This clinically relevant population of tumor cells can be evaluated by standard methods to investigate apoptotic, metabolic, and cell cycle regulatory pathways as well as providing a more rigorous target in which to test novel therapeutic strategies prior to pre-clinical investigations targeted at minimal residual disease.

Modeling Chemotherapy Resistant Leukemia In Vitro

The current report summarizes a protocol that can be utilized to model the influence of the bone marrow microenvironment niche on leukemic cells with emphasis placed on enrichment of the most chemoresistant subpopulation.

It is well established that the bone marrow microenvironment provides a unique site of sanctuary for hematopoietic diseases that both initiate and ...

Isolation of CD133+ Liver Stem Cells for Clonal Expansion

Liver stem cell, or oval cells, proliferate during chronic liver injury, and are proposed to differentiate into both hepatocytes and cholangiocytes. In addition, liver stem cells are hypothesized to be the precursors for a subset of liver cancer, Hepatocellular carcinoma. One of the primary challenges to stem cell work in any solid organ like the liver is the isolation of a rare population of cells for detailed analysis. For example, the vast majority of cells in the liver are hepatocytes (parenchymal fraction), which are significantly larger than non-parenchymal cells. By enriching the specific cellular compartments of the liver (i.e. parenchymal and non-parenchymal fractions), and selecting for CD45 negative cells, we are able to enrich the starting population of stem cells by over 600-fold.The proceduresdetailed in this report allow for a relatively rare population of cells from a solid organ to be sorted efficiently. This process can be utilized to isolateliver stem cells from normal murine liver as well as chronic liver injury models, which demonstrate increased liver stem cell proliferation. This method has clear advantages over standard immunohistochemistry of frozen or formalin fixed liver as functional studies using live cells can be performed after initial co-localization experiments. To accomplish the procedure outlined in this report, a working relationship with a research based flow-cytometry core is strongly encouraged as the details of FACS isolation are highly dependent on specialized instrumentation and a strong working knowledge of basic flow-cytometry procedures. The specific goal of this process is to isolate a population of liver stem cells that can be clonally expanded in vitro.

Here we describe the isolation of CD133 expressing liver stem cells and cancer stem cells from whole murine liver, a process that requires tissue digestion, cell enrichment, and flow cytometry isolation. We include methods for advanced single cell isolation and clonal expansion.

Liver stem cell, or oval cells, proliferate during chronic liver injury, and are proposed to differentiate into both hepatocytes and cholangiocytes. In ...

Biology

Chromosome Preparation From Cultured Cells

Chromosome (cytogenetic) analysis is widely used for the detection of chromosome instability. When followed by G-banding and molecular techniques such as fluorescence in situ hybridization (FISH), this assay has the powerful ability to analyze individual cells for aberrations that involve gains or losses of portions of the genome&#160;and rearrangements involving one or more chromosomes. In humans, chromosome abnormalities occur in approximately 1 per 160 live births1,2, 60-80% of all miscarriages3,4, 10% of stillbirths2,5, 13% of individuals with congenital heart disease6, 3-6% of infertility cases2, and in many patients with developmental delay&#160;and birth defects7. Cytogenetic analysis of malignancy is routinely used by researchers and clinicians, as observations of clonal chromosomal abnormalities have been shown to have both diagnostic and prognostic significance8,9.&#160; Chromosome isolation is invaluable for gene therapy and stem cell research of organisms including nonhuman primates and rodents10-13.
Chromosomes can be isolated from cells of live tissues, including blood lymphocytes, skin fibroblasts, amniocytes, placenta, bone marrow, and tumor specimens. Chromosomes are analyzed at the metaphase stage of mitosis, when they are most condensed and therefore more clearly visible. The first step of the chromosome isolation technique involves the disruption of the spindle fibers by incubation with Colcemid, to prevent the cells from proceeding to the subsequent anaphase stage. The cells are then treated with a hypotonic solution and preserved in their swollen state with Carnoy&#39;s fixative. The cells are then dropped on to slides and can then be utilized for a variety of procedures. G-banding involves trypsin treatment followed by staining with Giemsa to create characteristic light and dark bands. The same procedure to isolate chromosomes can be used for the preparation of cells for procedures such as fluorescence in situ hybridization (FISH), comparative genomic hybridization (CGH), and spectral karyotyping (SKY)14,15.

Chromosomes can be isolated from live cells such as lymphocytes or skin fibroblasts, and from organisms including humans or mice. These chromosome preparations can be further utilized for routine G-banding and molecular cytogenetic procedures such as fluorescence in situ hybridization (FISH), comparative genomic hybridization (CGH), and spectral karyotyping (SKY).

Chromosome (cytogenetic) analysis is widely used for the detection of chromosome instability. When followed by G-banding and molecular techniques such as ...

Density Gradient Centrifugation: A Method to Isolate CLL Cells from Peripheral Blood

Source: Hay, J. et al. <a href="https://www-jove-com.bdigitaluss.remotexs.co/t/60426">Subcellular Fractionation of Primary Chronic Lymphocytic Leukemia Cells to Monitor Nuclear/Cytoplasmic Protein Trafficking.</a> J. Vis. Exp. (2019).
This video describes the technique of isolating chronic lymphocytic leukemia (CLL) cells from peripheral blood. With this protocol, we will isolate CLL cells from human patient blood sample for subsequent efficient generation of nuclear and cytoplasmic fractions.

Source: Hay, J. et al. Subcellular Fractionation of Primary Chronic Lymphocytic Leukemia Cells to Monitor Nuclear/Cytoplasmic Protein Trafficking. J. Vis. ...

JoVE Encyclopedia of Experiments

Leukemia

Cell isolation & characterization

Preparation of Subcellular Fractions from Leukemic Cells: A Method to Generate Cellular and Nuclear Fractions from Leukemic Cells

Source: Hay, J., et al. <a href="https://www-jove-com.bdigitaluss.remotexs.co/t/60426">Subcellular Fractionation of Primary Chronic Lymphocytic Leukemia Cells to Monitor Nuclear/Cytoplasmic Protein Trafficking.</a> J. Vis. Exp. (2019).
This video describes the preparation of subcellular fractions from leukemic cells which is a method to generate cellular and nuclear fractions from leukemic cells. The nuclear and cytoplasmic fractions can be used for further downstream analysis.

Source: Hay, J., et al. Subcellular Fractionation of Primary Chronic Lymphocytic Leukemia Cells to Monitor Nuclear/Cytoplasmic Protein Trafficking. J. ...

In vitro techniques & assays

Leukemic Subpopulation Harvest: A Method for Spatial Separation of Leukemic Cell Subpopulations from 2D Co-culture

Source: Slone, W. L., et al. <a href="https://www-jove-com.bdigitaluss.remotexs.co/t/53645">Modeling Chemotherapy Resistant Leukemia In Vitro.</a> J. Vis. Exp. (2016).
This video describes a method for spatial separation of three leukemic cell subpopulations: the suspended leukemic cells freely floating in the media, phase bright leukemic cells adhered to the surface of the mesenchymal stromal cell monolayer, and the phase dim leukemic cells that have migrated beneath the mesenchymal stromal cell monolayer from 2D co-culture.

Source: Slone, W. L., et al. Modeling Chemotherapy Resistant Leukemia In Vitro. J. Vis. Exp. (2016).
This video describes a method for spatial separation ...

Preparation of Primary Acute Lymphoblastic Leukemia Cells in Different Cell Cycle Phases by Centrifugal Elutriation

Summary

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Chapters in this video

A Chromatin Immunoprecipitation Assay to Identify Novel NFAT2 Target Genes in Chronic Lymphocytic Leukemia

Subcellular Fractionation of Primary Chronic Lymphocytic Leukemia Cells to Monitor Nuclear/Cytoplasmic Protein Trafficking

From a 2DE-Gel Spot to Protein Function: Lesson Learned From HS1 in Chronic Lymphocytic Leukemia

A Simple Red Blood Cell Lysis Method for the Establishment of B Lymphoblastoid Cell Lines

Modeling Chemotherapy Resistant Leukemia In Vitro

Isolation of CD133+ Liver Stem Cells for Clonal Expansion

Chromosome Preparation From Cultured Cells

Density Gradient Centrifugation: A Method to Isolate CLL Cells from Peripheral Blood

Preparation of Subcellular Fractions from Leukemic Cells: A Method to Generate Cellular and Nuclear Fractions from Leukemic Cells

Leukemic Subpopulation Harvest: A Method for Spatial Separation of Leukemic Cell Subpopulations from 2D Co-culture