The authors thank Libby Perry (Augusta University) for her help with the SEM sample preparation. This work was supported by the National Institutes of Health [R01HL139562 (G.C.) and K99HL146954 (B.S.)] and American Heart Association [17POST33661254 (B.S.)].

NOTE: The following is a general protocol used to quantify membrane ruffle formation in RAW 264.7 macrophages using SEM microscopy. Optimization may be required for different cell types.
1. Cell line and cell culture
<ol>
	<li>Grow RAW 264.7 macrophages in Dulbecco&#39;s Modified Eagle Medium (DMEM) supplemented with 10% (vol/vol) heat-inactivated Fetal Bovine Serum (FBS), 100 IU/mL of penicillin and 100 &#181;g/mL streptomycin in a humidified incubator at 37 &#176;C and 5% CO2. Replace growth media every other day.</li>
	<li>When cells become 80% confluent, wash the plate two times using sterile PBS.</li>
	<li>Detach cells by adding 1,000 &#181;L of 0.5% trypsin-EDTA and incubate the cell culture plate for 3-5 min in a humidified incubator at 37 &#176;C.</li>
	<li>Examine the plate under a light microscope to confirm cell dissociation. Add 10 mL of growth media containing 10% FBS to inactivate trypsin.</li>
	<li>Collect the cell suspension in a 50 mL conical tube and centrifuge at 400 x g for 5 min at room temperature. Gently resuspend cells in the complete cell culture medium and determine the cell count and viability using Trypan Blue (0.4%) staining. 
	NOTE: The recommended minimum cell viability for this experiment is &#62;90%.</li>
	<li>Place sterile glass coverslips in wells of a 24-well plate using autoclaved forceps. Seed cells onto coverslips at a density of 1 x 106 cells/mL and incubate the plate overnight in a humidified incubator at 37 &#176;C and 5% CO2.</li>
	<li>Change media of each well with fresh 500 &#181;L complete media before treatment. Pretreat macrophages with vehicle (DMSO or other solvents used to dissolve EIPA) or the macropinocytosis inhibitor 5-(N-ethyl-N-isopropyl)-Amiloride (EIPA, 25 &#181;M21) for 30 min.</li>
	<li>Treat cells with vehicle and stimulators of macropinocytosis to promote membrane ruffling: phorbol 12-myristate 13-acetate (PMA, 1 &#181;M, 30 min21) and macrophage colony-stimulating factor (M-CSF, 100 ng/mL, 30 min3). 
	NOTE: Alternative inhibitors [e.g., latrunculin A (1 &#181;M, 30 min) or cytochalasin D (1 &#181;M, 30 min)] and stimulators [e.g., epidermal growth factor (EGF, 100 ng/mL, 10 min) or platelet-derived growth factor (PDGF, 100 ng/mL, 15 min)] of macropinocytosis can be also used to characterize macropinocytosis in macrophages and other cell types16,27,28,29. Cells may require overnight serum starvation prior to the treatment with physiological stimulators of macropinocytosis. It is important to note that the most effective concentrations and incubation times will have to be determined to stimulate macropinocytosis in other cell types.</li>
</ol>
2. SEM fixation
<ol>
	<li>After the treatment, aspirate the media from wells and wash coverslips with ice-cold PBS twice.</li>
	<li>Fix cells (4% paraformaldehyde and 2% glutaraldehyde in 0.1 M sodium cacodylate) for 30 min at room temperature, followed by overnight incubation in the fixative at 4 &#176;C.</li>
	<li>Gently wash and incubate coverslips with 500 &#181;L of following reagents without disturbing the cell monolayer.
	<ol>
		<li>Wash once in 0.1 M sodium cacodylate and incubate for 15 min.</li>
		<li>Wash twice with dH2O with 10 min incubation in each wash.</li>
		<li>Wash twice with 25% ethanol with 10 min incubation in each wash.</li>
		<li>Wash twice with 50% ethanol with 10 min incubation in each wash.</li>
		<li>Wash twice with 75% ethanol with 10 min incubation in each wash.</li>
		<li>Wash twice with 80% ethanol with 10 min incubation in each wash.</li>
		<li>Wash twice with 95% ethanol with 10 min incubation in each wash.</li>
		<li>Wash twice with 100% ethanol. Perform 10 min of incubation in each wash. 
		NOTE: Changing/replacing of reagents should be done fast to prevent air drying of cells. Coverslips can be left in 100% ethanol for several days at 4 &#176;C. For long-term storage, add additional 100% ethanol and cover wells with parafilm to prevent air drying of the sample.</li>
	</ol>
	</li>
</ol>
3.&#160;Critical point drying
<ol>
	<li>Place coverslips in a Critical Point Dryer and cover with 100% ethanol. Press the Power button and open the CO2 tank.</li>
	<li>Press the Cool button for approximately 30 s until the temperature decreases to 0 &#176;C. Press the Fill button until a bubble appears in the chamber window.</li>
	<li>Press the Purge button until the smell of ethanol from the purge exhaust disappears. Press the Cool button again until the temperature decreases to 0 &#176;C.</li>
	<li>Repress the Fill and Purge buttons to turn them off and close the CO2 tank. Repress the Cool button to turn it off and press the Heat button.</li>
	<li>Set the temperature at 42 &#176;C and pressure at 1,200 psi. Once the pressure and temperature stabilize, press the Bleed button to allow the pressure to decrease slowly.</li>
	<li>Once the chamber pressure reaches 150 psi, press the Vent button and wait until the pressure decreases to 0 psi. Turn off the critical point dryer and remove the coverslips.</li>
	<li>Mount coverslips on SEM aluminum specimen mounts using Carbon Adhesive tabs and subject to sputter coating using gold/palladium in a sputter coater.</li>
	<li>Turn on the Power button and wait until the vacuum reaches 30 mTorr. Flush the chamber to remove humidity and air by turning off the gas switch and turning the Fine gas valve counterclockwise.</li>
	<li>Once the vacuum increases to 200 mTorr turn off the gas switch and wait until the vacuum reaches 30 mTorr. Repeat this step 3 times.</li>
	<li>Push the Timer button and adjust the Voltage knob until the gauge reads 10 mA. Remove coated coverslips from the chamber. 
	NOTE: Follow manufacturer&#39;s instruction to perform critical point drying and sputter coating of the sample.</li>
</ol>
4. Imaging and quantification
<ol>
	<li>Insert sample coverslips into the chamber of a scanning electron microscope. Close the door and press the Evac button.</li>
	<li>Open the SEM operation software. Set the accelerating voltage to 15 kv and the working distance to 10 mm.</li>
	<li>Press the Coordinates button and move around the controller until the cells appear in the center of the observation screen. Set the magnification to 3,500x and image the sample by clicking the Photo button. 
	NOTE: Use a higher level of magnification (8,500x to 16,000x) to show the plasma membrane at greater details.</li>
	<li>Take images from at least 10 random locations on the coverslips, making sure that each microscopic field contains multiple cells. Save images as .tif files.</li>
	<li>From the images, locate membrane ruffles, defined as protruding blanket-like folds of the plasma membrane, with a size greater than 500 nm (Figure 1). Count the number of ruffles per cell. 
	NOTE: C-shaped ruffles were identified as curved membrane protrusions that did not fuse on their lateral ends [(Figure 1 (M-CSF treatment) and Figure 2B]. Fused circular membrane ruffles, prior to their closure, were identified as macropinocytotic cups (Figure 2C).</li>
	<li>Normalize the number of membrane ruffles to the total number of cells in the microscopic field evaluated. Repeat this analysis for the samples from each group.</li>
</ol>

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The authors declare no conflicts of interest.

The present SEM imaging protocol provides a tool to visualize and quantify membrane ruffle formation, circular protrusions, and macropinocytic cups on the cell surface in vitro. Although the current protocol focuses on macrophages, studies have shown that membrane ruffle formation also occurs on various other cell types including dendritic cells, fibroblasts, neurons, and cancer cells11,12,14,<sup class='xref...

Macropinocytosis is an endocytic process responsible for internalizing a large amount of extracellular fluid and its content via the formation of dynamic and actin-driven plasma membrane protrusions called membrane ruffles1. Many of these membrane ruffles form cups that close and fuse back onto the cell and separate from the plasma membrane as large, heterogeneous intracellular endosomes also known as macropinosomes1. Although macropinocytosis is induced by growth factors such as macrophage colony-stimulating factor (M-CSF) and epidermal growth factor (EGF) in a wide range of cell types, an additional unique, calcium-dependent process known as constitutive macropinocytosis has been also observed in innate immune cells2,3,4,5,6,7,8.
The ability of cells to internalize extracellular material via macropinocytosis has been shown to play an important role in a variety of physiological processes ranging from nutrient uptake to pathogen capture and antigen presentation9,10,11. However, because this process is non-selective and inducible, it has also been implicated in a number of pathological conditions. Indeed, previous studies suggested that macropinocytosis plays an important role in Alzheimer&#39;s disease, Parkinson&#39;s disease, cancer, nephrolithiasis and atherosclerosis12,13,14,15,16. Moreover, certain bacteria and viruses have shown to utilize macropinocytosis to gain entry into host cells and induce infection17,18. Interestingly, stimulation of macropinocytosis can be also exploited for targeted delivery of therapeutic agents in various disease conditions19,20.
Previous studies have explored macropinocytosis by quantifying internalized fluorescently-tagged fluid-phase markers in the absence and presence of pharmacological agents that inhibit macropinocytosis using flow cytometry and confocal imaging21,22. Currently available pharmacological tools that inhibit macropinocytosis are limited to and comprise of 1) actin polymerization inhibitors (cytochalasin D and latrunculins), 2) PI3K blockers (LY-290042 and wortmannin) and 3) inhibitors of sodium hydrogen exchangers (NHE) (amiloride and EIPA)5,14,15,23,24,25. However, because these inhibitors have endocytosis independent effects, it is difficult to selectively determine the contribution of macropinocytosis to solute uptake and disease pathogenesis especially in vivo21.
Scanning electron microscopy (SEM) is a type of electron microscope that produces ultra-high-resolution images of cells using a focused beam of electrons26. In macropinocytosis research, SEM imaging is regarded as the gold standard technique to visualize topographical and morphological characteristics of the plasma membrane, quantify membrane ruffle formation, and investigate their progression towards macropinosome internalization. Furthermore, scanning electron microscopy combined with the quantification of solute uptake, in the presence and absence of macropinocytosis blockers, provides a reliable strategy to examine macropinocytotic solute internalization in vitro. This paper provides a detailed protocol on how to prepare cells for SEM, visualize the cell surface, quantify ruffle formation, and examine their progress towards cup closure and macropinosome internalization.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>0.5% Trypsin-EDTA</td>
			<td>Gibco</td>
			<td>15400-054</td>
			<td></td>
		</tr>
		<tr>
			<td>2% Glutaraldehyde</td>
			<td>Electron Microscopy Sciences</td>
			<td>16320</td>
			<td></td>
		</tr>
		<tr>
			<td>4% Paraformaldehyde</td>
			<td>Santa Cruz Biotechnology</td>
			<td>281692</td>
			<td></td>
		</tr>
		<tr>
			<td>5-(N-ethyl-N-isopropyl)-Amiloride</td>
			<td>Sigma Life Science</td>
			<td>A3085</td>
			<td></td>
		</tr>
		<tr>
			<td colspan="2">Accuri C6 Flow Cytometer</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Carbon Adhesive Tabs</td>
			<td>Electron Microscopy Sciences</td>
			<td>77825-09</td>
			<td></td>
		</tr>
		<tr>
			<td>Dimethyl Sulfoxide</td>
			<td>Corning</td>
			<td>25-950-CQC</td>
			<td></td>
		</tr>
		<tr>
			<td>Dulbecco&#39;s Modified Eagle Medium</td>
			<td>Cytiva Life Sciences</td>
			<td>SH30022.01</td>
			<td></td>
		</tr>
		<tr>
			<td>Falcon 24-well Clear Flat Bottom TC-treated Multiwell Cell Culture Plate</td>
			<td>Falcon</td>
			<td>353047</td>
			<td></td>
		</tr>
		<tr>
			<td>Fetal Bovine Serum</td>
			<td>Gemini Bio</td>
			<td>900-108</td>
			<td></td>
		</tr>
		<tr>
			<td>FitC-dextran</td>
			<td>Thermo Fisher Scientific</td>
			<td>D1823</td>
			<td></td>
		</tr>
		<tr>
			<td>FM 4-64</td>
			<td>Thermo Fisher Scientific</td>
			<td>T13320</td>
			<td></td>
		</tr>
		<tr>
			<td>HERAcell 150i CO2 incubator</td>
			<td>Thermo Fisher Scientific</td>
			<td>51026282</td>
			<td></td>
		</tr>
		<tr>
			<td>Hummer Model 6.2 Sputter Coater</td>
			<td>Anatech USA</td>
			<td>58565</td>
			<td></td>
		</tr>
		<tr>
			<td colspan="2">JSM-IT500HR scanning electron microscope</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Microscope Cover Glass</td>
			<td>Thermo Fisher Scientific</td>
			<td>12-545-82</td>
			<td></td>
		</tr>
		<tr>
			<td>Pen Strep</td>
			<td>Gibco</td>
			<td>15140-122</td>
			<td></td>
		</tr>
		<tr>
			<td>phorbol 12-myristate 13-acetate</td>
			<td>Millipore Sigma</td>
			<td>524400</td>
			<td></td>
		</tr>
		<tr>
			<td>RAW 264.7 macrophage</td>
			<td>ATCC</td>
			<td>ATCC TIB-71</td>
			<td></td>
		</tr>
		<tr>
			<td>Recombinant Human M-CSF</td>
			<td>Peprotech</td>
			<td>300-25</td>
			<td></td>
		</tr>
		<tr>
			<td>Samdri-790 Critical Point Dryer</td>
			<td>Tousimis Research Corporation</td>
			<td>8778B</td>
			<td></td>
		</tr>
		<tr>
			<td>SEM Aluminum Specimen Mounts</td>
			<td>Electron Microscopy Sciences</td>
			<td>75220</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium Cacodylate</td>
			<td>Electron Microscopy Sciences</td>
			<td>12300</td>
			<td></td>
		</tr>
		<tr>
			<td>Texas red-dextra</td>
			<td>Thermo Fisher Scientific</td>
			<td>D1864</td>
			<td></td>
		</tr>
		<tr>
			<td>Trypan Blue Solution</td>
			<td>Thermo Fisher Scientific</td>
			<td>15250061</td>
			<td></td>
		</tr>
		<tr>
			<td>Zeiss LSM 780 confocal microscope</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
	</tbody>
</table>

visualizing membrane ruffle formation using scanning electron microscopy

Membrane ruffling is the formation of motile plasma membrane protrusions containing a meshwork of newly polymerized actin filaments. Membrane ruffles may form spontaneously or in response to growth factors, inflammatory cytokines, and phorbol esters. Some of the membrane protrusions may reorganize into circular membrane ruffles that fuse at their distal margins and form cups that close and separate into the cytoplasm as large, heterogeneous vacuoles called macropinosomes. During the process, ruffles trap extracellular fluid and solutes that internalize within macropinosomes. High-resolution scanning electron microscopy (SEM) is a commonly used imaging technique to visualize and quantify membrane ruffle formation, circular protrusions, and closed macropinocytic cups on the cell surface. The following protocol describes the cell culture conditions, stimulation of the membrane ruffle formation in vitro, and how to fix, dehydrate, and prepare cells for imaging using SEM. Quantification of membrane ruffling, data normalization, and stimulators and inhibitors of membrane ruffle formation are also described. This method can help answer key questions about the role of macropinocytosis in physiological and pathological processes, investigate new targets that regulate membrane ruffle formation, and identify yet uncharacterized physiological stimulators as well as novel pharmacological inhibitors of macropinocytosis.

Here, we describe the results from the presented technique. Representative SEM images shown in Figure 1 demonstrate membrane ruffle formation in RAW 264.7 macrophages following treatment with PMA and M-CSF. Images were first captured at a magnification of 3,500x for quantification purposes and then at higher levels of magnification (8,500x to 16,000x) to show the plasma membrane at greater details. Pretreatment of macrophages with the macropinocytosis inhibitor EIPA attenuated membrane ruffl...

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Visualizing Membrane Ruffle Formation using Scanning Electron Microscopy

Macropinocytosis is a highly conserved endocytic process initiated by the formation of F-actin-rich sheet-like membrane projections, also known as membrane ruffles. Increased rate of macropinocytotic solute internalization has been implicated in various pathological conditions. This protocol presents a method to quantify membrane ruffle formation in vitro using scanning electron microscopy.

Membrane ruffling is the formation of motile plasma membrane protrusions containing a meshwork of newly polymerized actin filaments. Membrane ruffles may ...

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Research

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Medicine

2.4K Views.  Medical College of Georgia at Augusta University. Macropinocytosis is a highly conserved endocytic process initiated by the formation of F-actin-rich sheet-like membrane projections, also known as membrane ruffles. Increased rate of macropinocytotic solute internalization has been implicated in various pathological conditions. This protocol presents a method to quantify membrane ruffle formation in vitro using scanning electron microscopy. 

Video: Visualizing Membrane Ruffle Formation using Scanning Electron Microscopy

Oral Biofilm Analysis of Palatal Expanders by Fluorescence In-Situ Hybridization and Confocal Laser Scanning Microscopy

Confocal laser scanning microscopy (CLSM) of natural heterogeneous biofilm is today facilitated by a comprehensive range of staining techniques, one of them being fluorescence in situ hybridization (FISH).1,2 We performed a pilot study in which oral biofilm samples collected from fixed orthodontic appliances (palatal expanders) were stained by FISH, the objective being to assess the three-dimensional organization of natural biofilm and plaque accumulation.3,4 FISH creates an opportunity to stain cells in their native biofilm environment by the use of fluorescently labeled 16S rRNA-targeting probes.4-7,19 Compared to alternative techniques like immunofluorescent labeling, this is an inexpensive, precise and straightforward labeling technique to investigate different bacterial groups in mixed biofilm consortia.18,20 General probes were used that bind to Eubacteria (EUB338 + EUB338II + EUB338III; hereafter EUBmix),8-10 Firmicutes (LGC354 A-C; hereafter LGCmix),9,10 and Bacteroidetes (Bac303).11 In addition, specific probes binding to Streptococcus mutans (MUT590)12,13 and Porphyromonas gingivalis (POGI)13,14 were used. The extreme hardness of the surface materials involved (stainless steel and acrylic resin) compelled us to find new ways of preparing the biofilm. As these surface materials could not be readily cut with a cryotome, various sampling methods were explored to obtain intact oral biofilm. The most workable of these approaches is presented in this communication. Small flakes of the biofilm-carrying acrylic resin were scraped off with a sterile scalpel, taking care not to damage the biofilm structure. Forceps were used to collect biofilm from the steel surfaces. Once collected, the samples were fixed and placed directly on polysine coated glass slides. FISH was performed directly on these slides with the probes mentioned above. Various FISH protocols were combined and modified to create a new protocol that was easy to handle.5,10,14,15 Subsequently the samples were analyzed by confocal laser scanning microscopy. Well-known configurations3,4,16,17 could be visualized, including mushroom-style formations and clusters of coccoid bacteria pervaded by channels. In addition, the bacterial composition of these typical biofilm structures were analyzed and 2D and 3D images created.

We present a protocol for structural and compositional analysis of natural oral biofilm from orthodontic appliances with in situ hybridization (FISH) and confocal laser scanning microscopy (CLSM). Oral biofilm samples were collected from palatal expanders, scraping acrylic-resin flakes off their surface and referring them for molecular processing.

Confocal laser scanning microscopy (CLSM) of natural heterogeneous biofilm is today facilitated by a comprehensive range of staining techniques, one of ...

Formation of Human Prostate Epithelium Using Tissue Recombination of Rodent Urogenital Sinus Mesenchyme and Human Stem Cells

Progress in prostate cancer research is severely limited by the availability of human-derived and hormone-na&iuml;ve model systems, which limit our ability to understand genetic and molecular events underlying prostate disease initiation. Toward developing better model systems for studying human prostate carcinogenesis, we and others have taken advantage of the unique pro-prostatic inductive potential of embryonic rodent prostate stroma, termed urogenital sinus mesenchyme (UGSM). When recombined with certain pluripotent cell populations such as embryonic stem cells, UGSM induces the formation of normal human prostate epithelia in a testosterone-dependent manner. Such a human model system can be used to investigate and experimentally test the ability of candidate prostate cancer susceptibility genes at an accelerated pace compared to typical rodent transgenic studies. Since Human embryonic stem cells (hESCs) can be genetically modified in culture using inducible gene expression or siRNA knock-down vectors prior to tissue recombination, such a model facilitates testing the functional consequences of genes, or combinations of genes, which are thought to promote or prevent carcinogenesis.
The technique of isolating pure populations of UGSM cells, however, is challenging and learning often requires someone with previous expertise to personally teach. Moreover, inoculation of cell mixtures under the renal capsule of an immunocompromised host can be technically challenging. Here we outline and illustrate proper isolation of UGSM from rodent embryos and renal capsule implantation of tissue mixtures to form human prostate epithelium. Such an approach, at its current stage, requires in vivo xenografting of embryonic stem cells; future applications could potentially include in vitro gland formation or the use of induced pluripotent stem cell populations (iPSCs).

To unravel the earliest molecular mechanisms underlying prostate cancer initiation, novel and innovative human model systems and approaches are desperately needed. The potential of pre-prostatic urogenital sinus mesenchyme (UGSM) to induce pluripotent stem cell populations to form human prostate epithelium is a powerful experimental tool in prostate research.

Progress in prostate cancer research is severely  limited by the availability of human-derived and hormone-na&iuml;ve model systems,  which limit our ...

Quantitative Visualization of Leukocyte Infiltrate in a Murine Model of Fulminant Myocarditis by Light Sheet Microscopy

Light-sheet fluorescence microscopy (LSFM), in combination with chemical clearing protocols, has become the gold standard for analyzing fluorescently labelled structures in large biological specimens, and is down to cellular resolution. Meanwhile, the constant refinement of underlying protocols and the enhanced availability of specialized commercial systems enable us to investigate the microstructure of whole mouse organs and even allow for the characterization of cellular behavior in various live-cell imaging approaches. Here, we describe a protocol for the spatial whole-mount visualization and quantification of the CD45+ leukocyte population in inflamed mouse hearts. The method employs a transgenic mouse strain (CD11c.DTR)that has recently been shown to serve as a robust, inducible model for the study of the development of fulminant fatal myocarditis, characterized by lethal cardiac arrhythmias. This protocol includes myocarditis induction, intravital antibody-mediated cell staining, organ preparation, and LSFM with subsequent computer-assisted image post-processing. Although presented as a highly-adapted method for our particular scientific question, the protocol represents the blueprint of an easily adjustable system that can also target completely different fluorescent structures in other organs and even in other species.

Here, we describe a light-sheet microscopy approach to visualize the cardiac CD45+ leukocyte infiltrate in a murine model of aseptic fulminant myocarditis, which is induced by the intratracheal diphtheria toxin treatment of CD11c.DTR mice.

Light-sheet fluorescence microscopy (LSFM), in combination with chemical clearing protocols, has become the gold standard for analyzing fluorescently ...

Preparation and In Vitro Characterization of Magnetized miR-modified Endothelial Cells

To date, the available surgical and pharmacological treatments for cardiovascular diseases (CVD) are limited and often palliative. At the same time, gene and cell therapies are highly promising alternative approaches for CVD treatment. However, the broad clinical application of gene therapy is greatly limited by the lack of suitable gene delivery systems. The development of appropriate gene delivery vectors can provide a solution to current challenges in cell therapy. In particular, existing drawbacks, such as limited efficiency and low cell retention in the injured organ, could be overcome by appropriate cell engineering (i.e., genetic) prior to transplantation. The presented protocol describes the efficient and safe transient modification of endothelial cells using a polyethyleneimine superparamagnetic magnetic nanoparticle (PEI/MNP)-based delivery vector. Also, the algorithm and methods for cell characterization are defined. The successful intracellular delivery of microRNA (miR) into human umbilical vein endothelial cells (HUVECs) has been achieved without affecting cell viability, functionality, or intercellular communication. Moreover, this approach was proven to cause a strong functional effect in introduced exogenous miR. Importantly, the application of this MNP-based vector ensures cell magnetization, with accompanying possibilities of magnetic targeting and non-invasive MRI tracing. This may provide a basis for magnetically guided, genetically engineered cell therapeutics that can be monitored non-invasively with MRI.

Preparation and In Vitro Characterization of Magnetized miR-modified Endothelial Cells

This manuscript describes the efficient, non-viral delivery of miR to endothelial cells by a PEI/MNP vector and their magnetization. Thus, in addition to genetic modification, this approach allows for magnetic cell guidance and MRI detectability. The technique can be used to improve the characteristics of therapeutic cell products.

To date, the available surgical and pharmacological treatments for cardiovascular diseases (CVD) are limited and often palliative. At the same time, gene ...

Micro-dissection of Enamel Organ from Mandibular Incisor of Rats Exposed to Environmental Toxicants

Enamel defects resulting from environmental conditions and ways of life are public health concerns because of their high prevalence. These defects result from altered activity of cells responsible for enamel synthesis named ameloblasts, which present in enamel organ. During amelogenesis, ameloblasts follow a specific and precise sequence of events of proliferation, differentiation, and death. A rat continually growing incisors is a suitable experimental model to study ameloblast activity and differentiation stages in physiological and pathological conditions. Here, we describe a reliable and consistent method to micro-dissect enamel organ of rats exposed to environmental toxicants. The micro-dissected dental epithelia contain secretion- and maturation-stage ameloblasts that may be used for qualitative experiments, such as immunohistochemistry assays and in situ hybridization, as well as for quantitative analyses such as RT-qPCR, RNA-seq, and Western blotting.

Understanding enamel formation and possible alterations requires the study of ameloblast activity. Here, we describe a reliable and consistent method to micro-dissect enamel organs containing secretion- and maturation-stage ameloblasts that may be used for further quantitative and qualitative experimental procedures.

Enamel defects resulting from environmental conditions and ways of life are public health concerns because of their high prevalence. These defects result ...

Noninvasive Determination of Vortex Formation Time Using Transesophageal Echocardiography During Cardiac Surgery

Trans-mitral blood flow produces a three-dimensional rotational body of fluid, known as a vortex ring, that enhances the efficiency of left ventricular (LV) filling compared with a continuous linear jet. Vortex ring development is most often quantified with vortex formation time (VFT), a dimensionless parameter based on fluid ejection from a rigid tube. Our group is interested in factors that affect LV filling efficiency during cardiac surgery. In this report, we describe how to use standard two-dimensional (2D) and Doppler transesophageal echocardiography (TEE) to noninvasively derive the variables needed to calculate VFT. We calculate atrial filling fraction (&#946;) from velocity-time integrals of trans-mitral early LV filling and atrial systole blood flow velocity waveforms measured in the mid-esophageal four-chamber TEE view. Stroke volume (SV) is calculated as the product of the diameter of the LV outflow track measured in the mid-esophageal long axis TEE view and the velocity-time integral of blood flow through the outflow track determined in the deep transgastric view using pulse-wave Doppler. Finally, mitral valve diameter (D) is determined as the average of major and minor axis lengths measured in orthogonal mid-esophageal bicommissural and long axis imaging planes, respectively. VFT is then calculated as 4 &#215; (1-&#946;) &#215; SV/(&#960;D3). We have used this technique to analyze VFT in several groups of patients with differing cardiac abnormalities. We discuss our application of this technique and its potential limitations and also review our results to date. Noninvasive measurement of VFT using TEE is straightforward in anesthetized patients undergoing cardiac surgery. The technique may allow cardiac anesthesiologists and surgeons to assess the impact of pathological conditions and surgical interventions on LV filling efficiency in real time.

We describe a protocol to measure vortex formation time, an index of left ventricular filling efficiency, using standard transesophageal echocardiography techniques in patients undergoing cardiac surgery. We apply this technique to analyze vortex formation time in several groups of patients with differing cardiac pathologies.

Trans-mitral blood flow produces a three-dimensional rotational body of fluid, known as a vortex ring, that enhances the efficiency of left ventricular ...

Using Q Suture to Enhance Resistance to Gap Formation and Tensile Strength of Repaired Flexor Tendons

Peripheral epitendinous sutures are believed to enhance core suture strength in tendon repair and decrease the risk of gapping between tendon ends. Here Q suture, an alternative to peripheral sutures, is presented for the use in tendon repair. Its effects on gap formation and tensile strength of the repaired tendons were compared with conventional running peripheral sutures. Three 2-strand sutures and three 4-strand sutures were used in repairing porcine tendons. The time required for performing 2Q and running sutures were recorded. The repaired tendons were subjected to a cyclic loading test, and the cycle number, during which a 2-mm gap was formed, was determined. After the cyclic loading, the gap size at the tendon ends and the ultimate strength of the repaired tendons were measured. Augmentation with the Q sutures reduced the number of tendons showing 2-mm gaps at tendon ends during cyclic loading. With addition of Q sutures 2-strand sutures significantly increased the ultimate strength of the repaired tendons and 4-strand sutures decreased the gap distance at the repair site of tendons. The time required for performing 2Q sutures was significantly less than that for running sutures. Therefore, we conclude that the Q suture is efficient in enhancing the tensile resistance and tendon repair strength and can be an alternative to conventional peripheral sutures.

Here, we present a &#8220;Q&#8221; suture technique that can be performed in tendon repair and its effects on the gap formation and tensile strength of the repaired tendons. Q suture is shown to be efficient in enhancing the tensile resistance and tendon repair strength.

Peripheral epitendinous sutures are believed to enhance core suture strength in tendon repair and decrease the risk of gapping between tendon ends. Here Q ...

Visualizing and Quantifying Pharmaceutical Compounds within Skin using Coherent Raman Scattering Imaging

Cutaneous pharmacokinetics (cPK) after topical formulation application has been a research area of particular interest for regulatory and drug development scientists to mechanistically understand topical bioavailability (BA). Semi-invasive techniques, such as tape-stripping, dermal microdialysis, or dermal open-flow microperfusion, all quantify macroscale cPK. While these techniques have provided vast cPK knowledge, the community lacks a mechanistic understanding of active pharmaceutical ingredient (API) penetration and permeation at the cellular level. 
One noninvasive approach to address microscale cPK is coherent Raman scattering imaging (CRI), which selectively targets intrinsic molecular vibrations without the need for extrinsic labels or chemical modification. CRI has two main methods-coherent anti-Stokes Raman scattering (CARS) and stimulated Raman scattering (SRS)-that enable sensitive and selective quantification of APIs or inactive ingredients. CARS is typically utilized to derive structural skin information or visualize chemical contrast. In contrast, the SRS signal, which is linear with molecular concentration, is used to quantify APIs or inactive ingredients within skin stratifications. 
Although mouse tissue has commonly been utilized for cPK with CRI, topical BA and bioequivalence (BE) must ultimately be assessed in human tissue before regulatory approval. This paper presents a methodology to prepare and image ex vivo skin to be used in quantitative pharmacokinetic CRI studies in the evaluation of topical BA and BE. This methodology enables reliable and reproducible API quantification within human and mouse skin over time. The concentrations within lipid-rich and lipid-poor compartments, as well as total API concentration over time are quantified; these are utilized for estimates of micro- and macroscale BA and, potentially, BE.

A coherent Raman scattering imaging methodology to visualize and quantify pharmaceutical compounds within the skin is described. This paper describes skin tissue preparation (human and mouse) and topical formulation application, image acquisition to quantify spatiotemporal concentration profiles, and preliminary pharmacokinetic analysis to assess topical drug delivery.

Cutaneous pharmacokinetics (cPK) after topical formulation application has been a research area of particular interest for regulatory and drug development ...

Ferric Chloride-Induced Arterial Thrombosis and Sample Collection for 3D Electron Microscopy Analysis

Cardiovascular diseases are a leading cause of mortality and morbidity worldwide. Aberrant thrombosis is a common feature of systemic conditions like diabetes and obesity, and chronic inflammatory diseases like atherosclerosis, cancer, and autoimmune diseases. Upon vascular injury, usually the coagulation system, platelets, and endothelium act in an orchestrated manner to prevent bleeding by forming a clot at the site of the injury. Abnormalities in this process lead to either excessive bleeding or uncontrolled thrombosis/insufficient antithrombotic activity, which translates into vessel occlusion and its sequelae. The FeCl3-induced carotid injury model is a valuable tool in probing how thrombosis initiates and progresses in vivo. This model involves endothelial damage/denudation and subsequent clot formation at the injured site. It provides a highly sensitive, quantitative assay to monitor vascular damage and clot formation in response to different degrees of vascular damage. Once optimized, this standard technique can be used to study the molecular mechanisms underlying thrombosis, as well as the ultrastructural changes in platelets in a growing thrombus. This assay is also useful to study the efficacy of antithrombotic and antiplatelet agents. This article explains how to initiate and monitor FeCl3-induced arterial thrombosis and how to collect samples for analysis by electron microscopy.

The present protocol describes how to use a FeCl3-mediated injury to induce arterial thrombosis, and how to collect and prepare arterial injury samples at various stages of thrombosis for electron microscopy analysis.

Cardiovascular diseases are a leading cause of mortality and morbidity worldwide. Aberrant thrombosis is a common feature of systemic conditions like ...

Advanced CAD Imaging for Surgical Margin Analysis in Cancer Care

Enhanced Communication of Tumor Margins Using 3D Scanning and Mapping

After oncologic resection of malignant tumors, specimens are sent to pathology for processing to determine the surgical margin status. These results are communicated in the form of a written pathology report. The current standard-of-care pathology report provides a written description of the specimen and the sites of margin sampling without any visual representation of the resected tissue. The specimen itself is typically destroyed during sectioning and analysis. This often leads to challenging communication between pathologists and surgeons when the final pathology report is confirmed. Furthermore, surgeons and pathologists are the only members of the multidisciplinary cancer care team to visualize the resected cancer specimen. We have developed a 3D scanning and specimen mapping protocol to address this unmet need. Computer-aided design (CAD) software is used to annotate the virtual specimen clearly showing sites of inking and margin sampling. This map can be utilized by various members of the multidisciplinary cancer care team.

Author Spotlight: 3D Scanning and Augmented Reality for Enhanced Cancer Surgery Communication

A novel method for 3D scanning and virtual mapping of cancer resections is proposed with the goal of improving communication among the multidisciplinary cancer care team.

After oncologic resection of malignant tumors, specimens are sent to pathology for processing to determine the surgical margin status. These results are ...