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24 pages, 19590 KiB  
Review
Multiphoton Tomography in Cosmetic Research
by Karsten König and Aisada König
Cosmetics 2025, 12(2), 44; https://doi.org/10.3390/cosmetics12020044 - 4 Mar 2025
Viewed by 141
Abstract
Background: Multiphoton tomography (MPT) is a femtosecond laser imaging technique that enables high-resolution virtual biopsies of human skin. It provides a non-invasive method for analyzing cellular metabolism, structural changes, and responses to cosmetic products, providing insights into cell–cosmetic interactions. This review explores the [...] Read more.
Background: Multiphoton tomography (MPT) is a femtosecond laser imaging technique that enables high-resolution virtual biopsies of human skin. It provides a non-invasive method for analyzing cellular metabolism, structural changes, and responses to cosmetic products, providing insights into cell–cosmetic interactions. This review explores the principles, historical development, and key applications of MPT in cosmetic research. Methods: The latest MPT device combines five modalities: (i) two-photon fluorescence: visualizes cells, elastin, and cosmetic ingredients; (ii) second harmonic generation (SHG): maps the collagen network; (iii) fluorescence lifetime imaging (FLIM): differentiates eumelanin from pheomelanin and evaluates the impact of cosmetics on cellular metabolic activity; (iv) reflectance confocal microscopy (RCM): images cell membranes and cosmetic particles; and (v) white LED imaging for dermoscopy. Results: MPT enables in-depth examination of extracellular matrix changes, cellular metabolism, and melanin production. It identifies skin responses to cosmetic products and tracks the intratissue distribution of sunscreen nanoparticles, nano- and microplastics, and other cosmetic components. Quantitative measurements, such as the elastin-to-collagen ratio, provide insights into anti-aging effects. Conclusions: MPT is a powerful in vivo imaging tool for the cosmetic industry. Its superior resolution and metabolic information facilitate the evaluation of product efficacy and support the development of personalized skincare solutions. Full article
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<p>The scheme illustrates two-photon fluorescence, e.g., from NADH, excited with near infrared light at 780 nm (<b>left</b>), and second harmonic generation (SHG), e.g., from collagen, at half the laser wavelength (doubling the laser frequency) (<b>right</b>). Fluorescence occurs from the lowest vibrational level of the first real electronic state, S<sub>1</sub>. In SHG, two photons are upconverted to a single SHG photon by a virtual state of a non-centrosymmetric molecule.</p>
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<p>FLIM measurement of the living human epidermis using time-correlated single photon counting (TCSPC). (<b>left</b>) The fluorescence decay curve of a particular pixel illustrates counts of detected fluorescence photons in different time channels (blue dots). An χ<sup>2</sup> value of 1.07 confirms a good fit (red fitting curve) obtained by a biexponential approach with a mean autofluorescence lifetime of 940 picoseconds. (<b>right</b>) The FLIM image shows a color-coded map of fluorescence lifetimes, ranging from 200 ps (red, corresponds to temporal resolution) to 2000 ps (blue).</p>
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<p>The two MPT images illustrate two different perspectives of the human forearm skin: (<b>a</b>) The vertical plane (XZ) provides a cross-sectional view of the skin from the outermost layer stratum corneum down to the upper dermis with the red-depicted SHG signal. (<b>b</b>) The horizontal “en face” plane (XY) within the upper dermis demonstrates the elastin (green, autofluorescence) and collagen (red, SHG) at a depth of 100 µm. (<b>c</b>) The illustration shows the XY and XZ imaging planes in the context of the skin’s anatomy.</p>
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<p>The first two-photon skin imaging device: the multiphoton tomograph “DermaInspect”. This prototype was delivered to the Beiersdorf AG in Hamburg in 2001.</p>
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<p>Multiphoton tomographs MPT<span class="html-italic">flex</span> and MPT<span class="html-italic">flex</span>-CARS based on a water-chilled tunable femtosecond Ti:sapphire laser, beam delivery through an optical arm, and the 360° imaging head with up to four photon detectors for the measurements of two-photon excited autofluorescence, SHG, and RAMAN/CARS signals of lipids and water.</p>
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<p>The latest “Prism Award 2024” winning multimodal multiphoton tomograph MPT<span class="html-italic">compact</span> with its ultracompact fiber laser head, integrated into the imaging head. The optical arm and the chiller are no longer required. The tomograph can run on batteries.</p>
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<p>MPT interface. The interface “connects” the human subject with the tomograph via magnetic forces (<b>left</b>). Detailed schematic view (<b>right</b>). The focusing optic is facilitated by an immersion oil droplet for refractive index matching. The metal coupling ring with a cover glass is mounted on an adhesive ring. The round coverslip provides a transparent barrier and, together with a drop of immersion oil, reduces refractive index mismatch. The water droplet avoids air between the cover glass and skin and, therefore, enhances image quality.</p>
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<p>MPT images highlight differences in healthy skin (<b>a</b>) versus diseased skin (<b>b</b>). In the healthy stratum corneum, polygonal corneocytes lack nuclei. However, in diseased conditions (e.g., psoriasis, eczema, dermatitis), corneocytes (<b>b</b>) often retain nuclei, reflecting disrupted keratinocyte maturation. (<b>c</b>) The region of interest area highlights corneocytes with retained nuclei. The “stripes” in the first image reflect breathing artifacts.</p>
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<p>MPT en face sections out of a stack of images taken from a human forearm down to a tissue depth of 100 μm. Two-photon excited autofluorescence (green) and SHG (red) (overlay), and confocal reflection (RCM, blue) signals are used to visualize the epidermis and upper dermis. At 0 µm depth (s. corneum), the AF image reveals large, polygonal keratinized cells without nuclei. The stratum corneum is highly reflective, as seen in the RCM image. Skin folds are evident in both AF and RCM images. At 15 µm depth (s. granulosum), the granulated and reflective layer is visible. At 25 µm (s. spinosum), well-defined keratinocytes with bright, grainy fluorescent cytoplasm are seen in the AF images, attributed to organelles such as mitochondria. The dark nuclei lack fluorescence. RCM images show a honeycomb pattern. When imaging at 40–45 µm depth (s. basale), melanin-containing cells appear brighter due to the presence of melanin caps above their nuclei. These melanin caps are also visible in RCM images due to the high refractive index of melanin. A little bit deeper at 50 µm (s. basale), a mix of AF and SHG signals from collagen structures are recorded. When imaging the upper dermis at a depth of 65 µm (d. papillae), pronounced collagen fibers (red, SHG) and cells (green) are seen presenting the epidermal–dermal junction. At a depth of 100 µm (upper dermis), dense collagen fibrils (red) and the elastin networks (green) are seen, as well as a few mast cells.</p>
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<p>Time-lapse imaging of a single intratissue cell in the s. spinosum during oxygen inhalation over 2 h to monitor intracellular metabolic activity of a specific single cell. The cell is highlighted by the dotted region of interest (ROI). Images were captured at specific time points: before oxygen supply = 0 min, at 5–10 min, 30 min, 60 min, 120 min during oxygen inhalation, and after inhalation. The images demonstrate the possibility to track and to image a single intratissue cell over hours without significant motion artefacts.</p>
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<p>Melanin distribution in a hyperpigmented spot imaged by two-photon FLIM using the multiphoton tomograph MPT<span class="html-italic">compact</span>. Melanin with its short autofluorescence lifetime is false color-coded in red, while NADH, with longer AF lifetime values, is false color-coded in green. Melanin granules were found at different z-depths (5–65 µm).</p>
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<p>Microplastics in decorative cosmetic formulations were in vivo tracked in human skin using FLIM. (<b>a</b>) The FLIM of the blue/green region of interest (ROI) highlights the microplastic particle localized in the s. corneum. (<b>b</b>) A second “Glitter-free” blue ROI shows the surrounding skin autofluorescence for comparison. The color scale represents the mean fluorescence lifetime values from 0 to 4000 ps. (<b>c</b>) The FLIM histogram shows that the microplastic particle (solid line) has a nearly 0.5 ns shorter mean lifetime than the surrounding skin tissue (dashed line).</p>
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<p>MPT sections demonstrating the possibility of imaging cosmetics in situ in human skin with high submicron resolution. (<b>a</b>) AF + RCM images of a skin gel (Gel No. 6 Skin Equalizer, Premium Aesthetic GmbH, Germany). The strong blue RCM signal indicates an accumulation of the product particularly in skin wrinkles. (<b>b</b>) The FLIM images of a skin repair creme (Ultra Intense Hyaluronic Age Repair Cream, Dr. Joseph GmbH, Bruneck, Italy) reveal differences in the distribution of the creme and its impact on skin cell metabolism. The false color-coded images represent fluorescence lifetime values (0–4 ns), while the grayscale intensity scale corresponds to photon events. The dashed circles indicate region of interests (ROI). (<b>c</b>) AF + SHG imaging of a creme with collagen components (ActiVLayr<sup>®</sup> Premium Skin-Tight Real Collagen Film, DERMA Layr<sup>®</sup> Technology Inside, Seoul, Republic of Korea). SHG signals (red, white arrows) visualize the collagen distribution of collagen particles.</p>
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<p>Comparison of AF images of s. spinosum cells captured at 1 s scan time per 512 × 512 pixel frame (<b>a</b>) versus 6 s (<b>b</b>) that is typically used in MPT. The image quality with the preferred faster capture time can be significantly improved when employing AI, e.g., for “denoising”.</p>
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11 pages, 936 KiB  
Article
FLIM-Phasor Analysis (FLIM-ϕ) of Aβ-Induced Membrane Order Alterations: Towards a Cell-Based Biosensor for Early Alzheimer’s Disease Diagnosis
by Antonella Battisti, Maria Grazia Ortore, Silvia Vilasi and Antonella Sgarbossa
Micromachines 2025, 16(2), 234; https://doi.org/10.3390/mi16020234 - 19 Feb 2025
Viewed by 461
Abstract
Alzheimer’s disease (AD) is a progressive neurodegenerative disorder, and its early detection can be critical for a prompt intervention that can potentially slow down the disease progression and improve the patient’s quality of life. However, a diagnosis based solely on clinical symptoms can [...] Read more.
Alzheimer’s disease (AD) is a progressive neurodegenerative disorder, and its early detection can be critical for a prompt intervention that can potentially slow down the disease progression and improve the patient’s quality of life. However, a diagnosis based solely on clinical symptoms can be challenging, especially in the early stages, while the detection of specific biomarkers such as amyloid-β peptide (Aβ) and tau proteins can provide objective evidence for diagnosis. In this work, we explored the effects of Aβ peptide on cell membrane properties thanks to fluorescence lifetime imaging (FLIM) combined with the phasor analysis (FLIM-ϕ). The results showed that the membrane viscosity is altered by the presence of Aβ peptide and that cells experience this effect even at nanomolar concentrations of peptide. This considerable sensitivity opens up the possibility of envisioning a cell-based biosensor able to detect very low concentrations of Aβ in a biological fluid, thus enabling timely diagnosis and intervention. Full article
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<p>FLIM-ϕ images and phasor plot of Ge1L in U2OS cells. Left: Ge1L in the membrane of U2OS cells with (+Aβ) and without (ctrl) addition of Aβ 100 nM in the medium and intensity images of the selected cells. Scale bar: 20 µm. Center: phasor plot of Ge1L in cells treated with Aβ (red circle), control cells (green circle), reference phasors for Ge1L in L<sub>o</sub> and L<sub>d</sub> phases (pink squares) and background emission due to free Ge1L in the medium (cyan circle). Cursor colors in the phasor plot correspond to colors in the FLIM images. Right: fractional intensity calculator showing the calibration (green lines) and phasor clouds given with a minimum threshold set to 20 by the whole set of imaged cells with (top) or without (bottom) Aβ 100 nM.</p>
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<p>(<b>A</b>): L<sub>o</sub> fraction of control cells and cells treated with 50 nM or 100 nM Aβ-olig for 1 h. (<b>B</b>): L<sub>o</sub> fraction of control cells and cells treated with 100 nM Aβ-olig or Aβ-fib imaged immediately after treatment (t = 0) or after 1 h (t = 1 h).</p>
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18 pages, 8498 KiB  
Article
Characterizing Metabolic Shifts in Septic Murine Kidney Tissue Using 2P-FLIM for Early Sepsis Detection
by Stella Greiner, Mahyasadat Ebrahimi, Marko Rodewald, Annett Urbanek, Tobias Meyer-Zedler, Michael Schmitt, Ute Neugebauer and Jürgen Popp
Bioengineering 2025, 12(2), 170; https://doi.org/10.3390/bioengineering12020170 - 10 Feb 2025
Viewed by 579
Abstract
In this study, thin mouse kidney sections from healthy mice and those infected leading to acute and chronic sepsis were examined with two-photon excited fluorescence lifetime imaging (2P-FLIM) using the endogenous fluorescent coenzymes nicotinamide adenine dinucleotide (NADH) and flavin adenine dinucleotide (FAD). The [...] Read more.
In this study, thin mouse kidney sections from healthy mice and those infected leading to acute and chronic sepsis were examined with two-photon excited fluorescence lifetime imaging (2P-FLIM) using the endogenous fluorescent coenzymes nicotinamide adenine dinucleotide (NADH) and flavin adenine dinucleotide (FAD). The results presented show that this approach is a powerful tool for investigating cell metabolism in thin tissue sections. An adapted measurement routine was established for these samples by performing a spectral scan, identifying a combination of two excitation wavelengths and two detection ranges suitable for detailed scan images of NADH and FAD. Selected positions in thin slices of the renal cortex of nine mice (three healthy, three with chronic sepsis, and three with acute sepsis) were studied using 2P-FLIM. In addition, overview images were obtained using two-photon excited fluorescence (2PEF) intensity. This study shows that healthy kidney slices differ considerably from those with acute sepsis with regard to their fluorescence lifetime signatures. The latter shows a difference in metabolism between the inner and outer cortex, indicating that outer cortical tubular cells switch their metabolism from oxidative phosphorylation to glycolysis in kidneys from mice with acute sepsis and back in later stages, as seen for mice with chronic infections. These findings suggest that 2P-FLIM could serve as a powerful tool for early-stage sepsis diagnosis and monitoring metabolic recovery during treatment. Full article
(This article belongs to the Section Biosignal Processing)
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<p>Pseudo-color mean photon arrival time overview images of murine kidney tissue thin sections of healthy (H1, H2, H3), chronically (C1, C2, C3) and acutely septic (A1, A2, A3) mice show a variety of structures. The labeled squares indicate the location of previously measured detail images (o1, o2, o3: outer cortex positions; i1, i2, i3: inner cortex positions, described and discussed in <a href="#sec3dot4-bioengineering-12-00170" class="html-sec">Section 3.4</a>). The hue describes the mean photon arrival times (excitation 798 nm, detection 455–510 nm), whereas the brightness displays the detected photon number and was scaled for visibility on a per-image basis. The fluorescence intensity is higher in the outer region of the kidney, the renal cortex (co in sample H1), than in the inner one, the renal medulla (me in sample H1). The tiles missing for example in samples C1 and A3 are a result of photon saturation of the hybrid detector. Dashed squares indicate the position of the details of samples H1, C2 and A3 shown below. In these detailed images, the proximal and distal tubules are distinguishable by their mean photon arrival times with proximal tubules showing higher mean photon arrival times indicated by circles. Arrows indicate blood vessels, with colored arrows indicating structures in blood vessels with lower (purple) and higher (yellow) mean photon arrival times as a result of elevated collagen cross-linking in those areas with higher fluorescence lifetimes.</p>
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<p>Determination of optimal excitation and detection wavelengths. Spectral FLIM scan of a healthy sample (mice H2 in bins of 10 frames for two excitation wavelengths (711 nm in violet, 876 nm in orange). The normalized fluorescence intensity is shown in different detection ranges for the two excitation wavelengths and the difference between the two (711–876, pink) (<b>a</b>), together with the behavior of the relative amplitude <math display="inline"><semantics> <mrow> <msub> <mi>a</mi> <mn>1</mn> </msub> </mrow> </semantics></math>. (<b>b</b>) and the lifetimes <math display="inline"><semantics> <mrow> <msub> <mi>τ</mi> <mn>1</mn> </msub> </mrow> </semantics></math> (<b>c</b>) and <math display="inline"><semantics> <mrow> <msub> <mi>τ</mi> <mn>2</mn> </msub> </mrow> </semantics></math> (<b>d</b>). Adequate detection ranges (violet (NADH) and orange (FAD) rectangles) were chosen regarding sufficient fluorescence intensity and minimal variance in the fitted lifetimes and amplitudes. The mean values of the fluorescence lifetimes and relative amplitudes in the chosen detection ranges are shown as horizontal lines with a 3% deviation indicated by a rectangle showing that almost all relevant data points lay in this range. Outliers are accepted to achieve a sufficient number of detected photons. The mean values are additionally listed in <a href="#bioengineering-12-00170-t003" class="html-table">Table 3</a>, and the lifetimes were used as fixed parameters in the pixel-wise fit of the detailed images described in <a href="#sec3dot4-bioengineering-12-00170" class="html-sec">Section 3.4</a>.</p>
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<p>This overview of FLIRR detail images (<b>a</b>) and histograms of these images (<b>b</b>) shows no considerable differences between samples from healthy mice and those with chronic and acute sepsis. (<b>a</b>) The areas of different brightness, which encode the intensity ratio NADH/FAD and show different colors and, therefore, FLIRR are distinguishable. The different areas are those of the proximal and distal tubules. (<b>b</b>) The variance between the histograms is higher for the inner cortex positions than for the outer cortex positions, probably due to partial interlacing with renal medulla tissue. Furthermore, the variance between kidneys from different mice is higher for chronic and acute sepsis compared to healthy samples. This may be due to a different immune response between the mice. Sample C3 shows an exceptionally high degree of variation between different positions in the inner cortex, which might be attributed to the high level of damage induced by the comparatively high laser power in these samples, resulting in the formation of new fluorophores. To mitigate these effects in future studies, lower excitation powers and shorter exposure times should be considered. Additionally, alternative autofluorescence correction algorithms may help distinguish genuine metabolic shifts from laser-induced artifacts. This is supported by a considerable increase in the number of photons during the measurement (see <a href="#app1-bioengineering-12-00170" class="html-app">Table S3 in the Supplementary Material</a>). A change of FLIRR to lower values in the outer cortex of acutely septic mice can be observed but needs to be quantified.</p>
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<p>(<b>a</b>) The FLIRR histogram of sample H2-o3 (black) with a fit using a single Gaussian curve (violet) shows a deviation from a normal distribution. (<b>b</b>) A fit using the sum (violet) of two Gaussian curves (pink, orange) shows that the image comprises two regions, each exhibiting a normal distribution of FLIRR. These two regions can be attributed to the distal (<math display="inline"><semantics> <mrow> <msub> <mi>μ</mi> <mn>1</mn> </msub> </mrow> </semantics></math>) and proximal tubules (<math display="inline"><semantics> <mrow> <msub> <mi>μ</mi> <mn>2</mn> </msub> </mrow> </semantics></math>), as visible in <a href="#bioengineering-12-00170-f003" class="html-fig">Figure 3</a>. (<b>c</b>) Comparison of mean fitted FLIRR and its standard error in the distal and proximal tubules of each infection group in the inner and outer cortex shows differences between the inner and outer cortex of kidneys of mice infected with acute sepsis, indicating a metabolism change in this region of the kidneys of these specimens.</p>
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12 pages, 2022 KiB  
Article
Subcellular Compartmentalization of Glucose Mediated Insulin Secretion
by Zhongying Wang, Tatyana Gurlo, Leslie S. Satin, Scott E. Fraser and Peter C. Butler
Cells 2025, 14(3), 198; https://doi.org/10.3390/cells14030198 - 29 Jan 2025
Viewed by 1022
Abstract
Regulation of blood glucose levels depends on the property of beta cells to couple glucose sensing with insulin secretion. This is accomplished by the concentration-dependent flux of glucose through glycolysis and oxidative phosphorylation, generating ATP. The resulting rise in cytosolic ATP/ADP inhibits K [...] Read more.
Regulation of blood glucose levels depends on the property of beta cells to couple glucose sensing with insulin secretion. This is accomplished by the concentration-dependent flux of glucose through glycolysis and oxidative phosphorylation, generating ATP. The resulting rise in cytosolic ATP/ADP inhibits KATP channels, inducing membrane depolarization and Ca2+ influx, which prompts insulin secretion. Evidence suggests that this coupling of glucose sensing with insulin secretion may be compartmentalized in the submembrane regions of the beta cell. We investigated the subcellular responses of key components involved in this coupling and found mitochondria in the submembrane zone, some tethered to the cytoskeleton near capillaries. Using Fluorescent Lifetime Imaging Microscopy (FLIM), we observed that submembrane mitochondria were the fastest to respond to glucose. In the most glucose-responsive beta cells, glucose triggers rapid, localized submembrane increases in ATP and Ca2+ as synchronized ~4-min oscillations, consistent with pulsatile insulin release after meals. These findings are consistent with the hypothesis that glucose sensing is coupled with insulin secretion in the submembrane zone of beta cells. This zonal adaptation would enhance both the speed and energy efficiency of beta cell responses to glucose, as only a subset of the most accessible mitochondria would be required to trigger insulin secretion. Full article
(This article belongs to the Special Issue Cellular Mechanisms in Mitochondrial Function and Calcium Signaling)
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<p>Mitochondria in the submembrane zone of beta cells. We outlined the cytoskeleton in live INS823/13 beta cells (<b>A</b>–<b>D</b>) and primary mouse beta cells (<b>E</b>–<b>H</b>) with live dye for either actin or tubulin followed by abberior LIVE ORANGE mito staining to visualize the mitochondria. Using Leica SP8 confocal microscopy with an 86x/1.20 W objective, mitochondria were invariably present in the submembrane region. In some sections, there was a close interaction between mitochondria and protrusions of the submembrane cytoskeleton (white arrow in inset (<b>B</b>,<b>D</b>,<b>F</b>,<b>H</b>), corresponding to the white box in panel (<b>A</b>,<b>C</b>,<b>E</b>,<b>G</b>)), which was reminiscent of the mitochondrial tethering previously reported in neurons. Scale bar = 5 μm.</p>
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<p>Application of FLIM in beta cells following a glucose challenge reveals an early preferential metabolic trajectory to OxPhos in submembrane mitochondria. FLIM imaging of a representative primary mouse beta cell (<b>A</b>) at basal glucose concentration (4 mM) and 5 min after glucose stimulation (16 mM). Following glucose stimulation, there is a predominant transition to oxidative phosphorylation in the submembrane zone, color-coded as red, depicting increased bound/total NAD(P)H). The quantification of the change in the ratio of bound/total NAD(P)H by FLIM in the perinuclear versus the submembrane zone (<b>B</b>) is provided in 6 primary mouse beta cells 5 min after glucose stimulation. NAD(P)H FLIM signal was captured by 2-photon excitation at 740 nm and emission between 440 and 500 nm. Data are presented as mean ± SD; * <span class="html-italic">p</span> &lt; 0.05, Wilcoxon signed-rank test. Scale bar, 5 μm. Beta cells (n = 6) were from dispersed mouse islets obtained from three independent isolations.</p>
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<p>Early submembrane activation of oxidative phosphorylation is associated with apparent tethered mitochondria to the tubulin network. Microtubule network and a cilium are visualized in stacked Z plane images (<b>A</b>) of SIR-tubulin dye decorated representative primary mouse beta cell. In a single plane of section (<b>B</b>) of the same cell, FLIM imaging at basal glucose (4 mM) and 5 min after exposure to glucose stimulation (16 mM) reveals an early transition to OxPhos in a presumed mitochondrion closely associated with a tubulin enriched region (white arrowhead) consistent with early activation of submembrane tethered mitochondria. A cilium is identified (A) in the stacked images, and in this cell, there is no suggestion of early activation of OxPhos at the base of the cilium in response to glucose stimulation. Scale bar, 5 μm.</p>
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<p>Submembrane Ca<sup>2+</sup> and ATP responses to glucose stimulation in isolated beta cells. We monitored the relative submembrane and perinuclear levels of Ca<sup>2+</sup> and ATP in isolated primary beta cells at basal glucose (4 mM) and following glucose stimulation (16 mM). There was a wide variance between individual beta cells. In the more responsive cells, exemplified in <a href="#cells-14-00198-f004" class="html-fig">Figure 4</a>, there were clear ~4 min oscillations of both Ca<sup>2+</sup> and ATP that were promptly amplified in response to glucose stimulation predominantly in the submembrane zone. The arrow indicates the addition of glucose. Changes in ATP levels were measured using a Perceval-HR sensor (black trace), and changes in Ca<sup>2+</sup> level were measured using Fura Red (red trace).</p>
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<p>Beta cell capillary relationship and proposed revised glucose sensing insulin secretion model. To evaluate the putative submembrane mitochondria and vascular endothelium of adjacent capillaries in beta cells, we deployed transmission electron micrography of fixed mouse whole pancreas and identified sections that included sections of capillaries ((<b>A</b>), scale bar 500 nm; white box indicate the region displayed in (<b>B</b>,<b>C</b>)). In some sections of beta cells facing capillaries, submembrane mitochondria were closely affiliated with apparent membrane-associated tethers (<b>B</b>,<b>C</b>; scale bar 250 nm) consistent with prior studies of neuronal synapses. Based on the studies presented here, as well as studies published elsewhere, we propose a revision of the canonical model of beta cell glucose sensing coupled to insulin secretion (<b>D</b>). We propose that, at least in some beta cells, there is a microdomain at the capillary endothelium interface where glucose delivered by the adjacent capillary is metabolized to pyruvate in a concentration-dependent manner. Pyruvate is then accessed by submembrane tethered mitochondria to produce ATP that is delivered directly to local K<sub>ATP</sub> channels in the cell membrane. This prompts depolarization of the cell membrane and an influx of Ca<sup>2+</sup> to the submembrane zone, prompting exocytosis of primed docked insulin secretory vesicles. The locally high submembrane Ca<sup>2+</sup> is then taken up by the membrane-adjacent mitochondria, driving the Ca<sup>2+</sup>-dependent OxPhos enzymes to generate the next pulse of ATP. The latter is facilitated by the availability of ADP as ATP is consumed by repolarizing the cell membrane and priming and docking the next repertoire of insulin secretory vesicles to the cell membrane.</p>
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10 pages, 2538 KiB  
Article
Rapid Acquisition of High-Pixel Fluorescence Lifetime Images of Living Cells via Image Reconstruction Based on Edge-Preserving Interpolation
by Yinru Zhu, Yong Guo, Xinwei Gao, Qinglin Chen, Yingying Chen, Ruijie Xiang, Baichang Lin, Luwei Wang, Yuan Lu and Wei Yan
Biosensors 2025, 15(1), 43; https://doi.org/10.3390/bios15010043 - 13 Jan 2025
Viewed by 738
Abstract
Fluorescence lifetime imaging (FLIM) has established itself as a pivotal tool for investigating biological processes within living cells. However, the extensive imaging duration necessary to accumulate sufficient photons for accurate fluorescence lifetime calculations poses a significant obstacle to achieving high-resolution monitoring of cellular [...] Read more.
Fluorescence lifetime imaging (FLIM) has established itself as a pivotal tool for investigating biological processes within living cells. However, the extensive imaging duration necessary to accumulate sufficient photons for accurate fluorescence lifetime calculations poses a significant obstacle to achieving high-resolution monitoring of cellular dynamics. In this study, we introduce an image reconstruction method based on the edge-preserving interpolation method (EPIM), which transforms rapidly acquired low-resolution FLIM data into high-pixel images, thereby eliminating the need for extended acquisition times. Specifically, we decouple the grayscale image and the fluorescence lifetime matrix and perform an individual interpolation on each. Following the interpolation of the intensity image, we apply wavelet transformation and adjust the wavelet coefficients according to the image gradients. After the inverse transformation, the original image is obtained and subjected to noise reduction to complete the image reconstruction process. Subsequently, each pixel is pseudo-color-coded based on its intensity and lifetime, preserving both structural and temporal information. We evaluated the performance of the bicubic interpolation method and our image reconstruction approach on fluorescence microspheres and fixed-cell samples, demonstrating their effectiveness in enhancing the quality of lifetime images. By applying these techniques to live-cell imaging, we can successfully obtain high-pixel FLIM images at shortened intervals, facilitating the capture of rapid cellular events. Full article
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<p>Workflow of image reconstruction based on edge-preserving interpolation. The green boxes represent data processing operations. The colored, black-and-white, and gray rounded rectangles denote the lifetime information, intensity information, and gradient orientation information of the fluorescence lifetime images, respectively. The dashed blue box presents the workflow of the adopted edge-preserving interpolation method. The blue squares contain the data from the original low-resolution image, which are directly assigned to the odd rows and columns of the high-resolution image. The pink squares contain the data from the first step of interpolation, their calculation involving the surrounding 4 × 4 pixels of the original image, and these data are interpolated to the even rows and columns of the high-pixel image. The yellow squares contain data from the second step of interpolation, calculated based on a 5 × 5 neighborhood in the high-pixel image, and these data are distributed on the odd rows and even columns or even rows and odd columns of the high-resolution image.</p>
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<p>Fluorescence lifetime images of microsphere captured at a low resolution (LP) of 256 × 256 pix-els, processed using bicubic interpolation, reconstructed through EPIM, and acquired at a high resolution serving as the ground truth (GT), respectively.</p>
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<p>(<b>a</b>) Fluorescence lifetime image comparison of the LP, bicubic-interpolated, EPIM reconstruction, and GT images, divided by dotted lines. The amplification factor was set to 2. (<b>b</b>–<b>d</b>) ROIs of (<b>a</b>). (<b>e</b>) Fluorescence lifetime distribution histogram of (<b>a</b>). (<b>f</b>–<b>h</b>) Spatially resolved analysis at the white dashed line in (<b>b</b>), (<b>c</b>), and (<b>e</b>), respectively.</p>
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<p>(<b>a</b>) Fluorescence lifetime image comparison of the LP (128 × 128), bicubic-interpolated, EPIM reconstruction, and GT images, divided by dotted lines. (<b>b</b>–<b>d</b>) ROIs of (<b>a</b>). (<b>e</b>) Fluorescence lifetime distribution histogram of (<b>a</b>).</p>
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<p>(<b>a</b>) Fluorescence lifetime image of live cells. The mitochondria are marked. (<b>b</b>) Regions of interest of (<b>a</b>). These images were collected continuously, with the first one starting at 0 min and the interval between each start time being 1 min. White arrows: rapid alterations in mitochondrial characteristics can be observed.</p>
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20 pages, 3854 KiB  
Article
Fluorescence Lifetime Imaging of NAD(P)H in Patients’ Lymphocytes: Evaluation of Efficacy of Immunotherapy
by Diana V. Yuzhakova, Daria A. Sachkova, Anna V. Izosimova, Konstantin S. Yashin, Gaukhar M. Yusubalieva, Vladimir P. Baklaushev, Artem M. Mozherov, Vladislav I. Shcheslavskiy and Marina V. Shirmanova
Cells 2025, 14(2), 97; https://doi.org/10.3390/cells14020097 - 10 Jan 2025
Viewed by 662
Abstract
Background: The wide variability in clinical responses to anti-tumor immunotherapy drives the search for personalized strategies. One of the promising approaches is drug screening using patient-derived models composed of tumor and immune cells. In this regard, the selection of an appropriate in vitro [...] Read more.
Background: The wide variability in clinical responses to anti-tumor immunotherapy drives the search for personalized strategies. One of the promising approaches is drug screening using patient-derived models composed of tumor and immune cells. In this regard, the selection of an appropriate in vitro model and the choice of cellular response assay are critical for reliable predictions. Fluorescence lifetime imaging microscopy (FLIM) is a powerful, non-destructive tool that enables direct monitoring of cellular metabolism on a label-free basis with a potential to resolve metabolic rearrangements in immune cells associated with their reactivity. Objective: The aim of the study was to develop a patient-derived glioma explant model enriched by autologous peripheral lymphocytes and explore FLIM of the redox-cofactor NAD(P)H in living lymphocytes to measure the responses of the model to immune checkpoint inhibitors. Methods: The light microscopy, FLIM of NAD(P)H and flow cytometry were used. Results: The results demonstrate that the responsive models displayed a significant increase in the free NAD(P)H fraction α1 after treatment, associated with a shift towards glycolysis due to lymphocyte activation. The non-responsive models exhibited no alterations or a decrease in the NAD(P)H α1 after treatment. The FLIM data correlated well with the standard assays of immunotherapy drug response in vitro, including morphological changes, the T-cells activation marker CD69, and the tumor cell proliferation index Ki67. Conclusions: The proposed platform that includes tumor explants co-cultured with lymphocytes and the NAD(P)H FLIM assay represents a promising solution for the patient-specific immunotherapeutic drug screening. Full article
(This article belongs to the Section Cellular Metabolism)
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Graphical abstract

Graphical abstract
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<p>Characteristics of G-EXP-L model. (<b>A</b>) Phase contrast microscopy of patient-derived G-EXP-L model on days 4, 9, and 14 of cultivation. The components of the model are shown by the numerated arrows: 1—adherent tumor fragment, 2—adherent tumor cells, 3—lymphocytes. (<b>B</b>) Expression of the activation markers CD69 and CD25 in live CD4+ and CD8+ T-cells before and after co-culturing with glioma explants. Dot plots show the measurements for the individual patients (dots), and horizontal lines connect the values for the same patient before and on day 14 of co-culturing. (<b>C</b>) Expression of proliferation marker Ki67 in tumor explants before and on day 14 of co-culturing. Dot plots show the measurements for individual patients (dots), and horizontal lines connect the values for the same patient before and after co-culturing. Statistics: paired Student’s <span class="html-italic">t</span>-test. * Significant difference, <span class="html-italic">p</span> ≤ 0.05.</p>
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<p>FLIM of NAD(P)H in lymphocytes before and after co-culturing with glioma explants. (<b>A</b>) Representative FLIM images of lymphocytes before and after co-culturing. The long lifetime component of NAD(P)H τ<sub>2</sub>, the relative contribution of free NAD(P)H α<sub>1</sub>, and the mean lifetime τ<sub>m</sub> are shown. (<b>B</b>) Coupled comparisons of fluorescence decay parameters (τ<sub>2</sub>, α<sub>1</sub>, τ<sub>m</sub>) before and after co-culturing. Dots are the measurements for individual patients. Coupled comparisons of NAD(P)H-α<sub>1</sub> before and after co-culturing. Dots are the mean values for individual patients. Lines connect the values before and after co-culturing for the same patient. Statistics: paired Student’s <span class="html-italic">t</span>-test. * Significant difference, <span class="html-italic">p</span> ≤ 0.05.</p>
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<p>Phase contrast microscopy of patient-derived G-EXP-L model after treatment with immune checkpoint inhibitors on the days 4, 9, and 14 of cultivation. Examples of the morphological response: (<b>A</b>)—“no response” (patient G27, anti-CTLA-4 treatment), (<b>B</b>)—“partial response” (patient G20, anti-PD-1 treatment), (<b>C</b>)—“response” (patient G30, combination) treatment. Bars are indicated in the images.</p>
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<p>Expression of the activation marker CD69 in CD8+ or CD4+ T-lymphocytes in the G-EXP-L models after immunotherapy with anti-CTLA-4 (<b>A</b>), anti-PD-1 (<b>B</b>), or their combination (<b>C</b>). Dot plots show measurements for individual patients (dots) and SEM (horizontal lines). The red boxes indicate the cases of a significant rise in the percentage of CD69+ cells, either in the CD8+ T-cell subset or both CD8+ and CD4+ T-cells. Statistics: Mann–Whitney U test. * Significant difference, <span class="html-italic">p</span> ≤ 0.05.</p>
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<p>Expression of proliferative index Ki67 of glioma cells in the G-EXP-L models after immunotherapy with anti-CTLA-4 (<b>A</b>), anti-PD-1 (<b>B</b>) or their combination (<b>C</b>). Dot plots show measurements for individual patients (dots) and SEM (horizontal lines). The red boxes indicate the cases of a significant decrease in the percentage of Ki67+ glioma cells. Statistics: Mann–Whitney U test. * Significant difference, <span class="html-italic">p</span> ≤ 0.05.</p>
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<p>FLIM of NAD(P)H in lymphocytes from the G-EXP-L models after anti-CTLA-4, anti-PD-1 or combined (anti-CTLA-4 + anti-PD-1) treatment. (<b>A</b>) Representative FLIM images of lymphocytes from responding (patient G30) and non-responding (patient G27) models. The relative amplitude of free NAD(P)H α<sub>1</sub> is shown in the untreated and treated T cells. Scale bar is indicated on the images. (<b>B</b>) Quantification of NAD(P)H α<sub>1</sub> for individual patient-derived models. The graphs display the mean and SD (horizontal lines). Dots are the measurements for individual cells. The red boxes indicate the cases of a significant rise in NAD(P)H α<sub>1</sub>. Statistics: Student’s <span class="html-italic">t</span>-test. * Significant difference, <span class="html-italic">p</span> ≤ 0.05.</p>
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<p>The experimental workflow.</p>
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18 pages, 1409 KiB  
Article
Population Dynamics of the Crocodile Shark, Pseudocarcharias kamoharai, in the Tropical Equatorial Pacific Ocean, Ecuador
by Marcos Douglas Calle-Morán, Eugenio Alberto Aragón-Noriega, Ana Rosa Hernández-Téllez, Emigdio Marín-Enríquez, Javier Tovar-Ávila, Juan Francisco Arzola-González and Jorge Payán-Alejo
Fishes 2025, 10(1), 5; https://doi.org/10.3390/fishes10010005 - 26 Dec 2024
Viewed by 1287
Abstract
The objectives of this study were to determine the rates of natural mortality (M), fishing mortality (F), total mortality (Z), the exploitation rates (E), as well as the biological reference points (BRPs) and [...] Read more.
The objectives of this study were to determine the rates of natural mortality (M), fishing mortality (F), total mortality (Z), the exploitation rates (E), as well as the biological reference points (BRPs) and the annual removal rates (R) of the crocodile shark, Pseudocarcharias kamoharai, in the Ecuadorian Pacific. Thirty similar and different models were applied to determine all these rates. These equations were obtained from studies on teleost and chondrichthyan fish. The biological parameters, including age, growth, longevity, and reproduction, were obtained from the specialized literature based on the biology of P. kamoharai in Ecuadorian waters. These biological parameters were used in all the models considered here. The M estimations were 0.14 to 0.28 based on six models for chondrichthyans and osteichthyes. These values were similar to the six algorithms designed for cartilaginous fish, ranging from 0.16 to 0.35; for this reason, these mortality rates were considered low. The Z values ranged from 0.08 to 0.51; however, they were not considered given that the three estimations were less than M, and only the Z = 0.51 was considered. Given that Z = 0.51 and M = 0.24, an F = 0.27 was obtained by subtraction, indicating a low mortality by fishing. E had values between 0.21 and 0.53, which indicated overexploitation that exceeded the Eopt = 0.50 value. The obtained BRPs were Fopt = 0.10 and 0.12 and Flim = 0.16, which showed that the optimal fishing levels (best possible capture) to achieve long-term sustainable exploitation of the stock encompass 10 to 16% of the fishing effort applied for this species. However, the F surpassed this prudential range. The annual removal percentage (R = 21%) demonstrated that 21% of the population was being removed. Based on the biology and ecology of this species, all models applied in this study showed that P. kamoharai had low natural and fishing mortality rates and moderate total mortality; its exploitation rate exceeded the fishing limits. These values and their life history traits indicated that this shark species cannot tolerate any fishing level without threatening its populations. Full article
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<p>Geographic location of Santa Rosa of Salinas within the coastal profile of Continental Ecuador, Tropical Ecuadorian Pacific Ocean.</p>
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<p>Values of the instantaneous mortality rate (<span class="html-italic">M</span>) and annual natural mortality rate (<span class="html-italic">H<sub>M</sub></span>) of the crocodile shark, <span class="html-italic">Pseudocarcharias kamoharai</span>, in Pacific Ecuadorian waters estimated through diverse methods commonly used for osteichthyes and chondrichthyans. (1) Alverson and Carney [<a href="#B19-fishes-10-00005" class="html-bibr">19</a>], (2) Rickhter and Efanov [<a href="#B20-fishes-10-00005" class="html-bibr">20</a>], (3) Pauly [<a href="#B21-fishes-10-00005" class="html-bibr">21</a>], and (4–6) the three models by Jensen [<a href="#B22-fishes-10-00005" class="html-bibr">22</a>]. The dotted line represents the mean <span class="html-italic">M</span> and the continuous line the mean <span class="html-italic">H<sub>M</sub></span>.</p>
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<p>Estimations of the instantaneous rate of natural mortality (<span class="html-italic">M</span>) and the annual natural mortality rate (<span class="html-italic">H<sub>M</sub></span>) of the crocodile shark, <span class="html-italic">Pseudocarcharias kamoharai</span>, in Ecuadorian waters based on distinct models used specifically for cartilaginous fish. (1–2) Frisk et al. [<a href="#B23-fishes-10-00005" class="html-bibr">23</a>], (3–4) Then et al. [<a href="#B24-fishes-10-00005" class="html-bibr">24</a>], (5) Zhao et al. [<a href="#B25-fishes-10-00005" class="html-bibr">25</a>], and (6) from the literature related to sharks from the order Lamniformes. The yellow dotted line represents the mean <span class="html-italic">M</span>, and the blue continuous line is the mean <span class="html-italic">H<sub>M</sub></span>.</p>
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<p>The estimated exploitation rates of <span class="html-italic">Pseudocarcharias kamoharai</span> in Ecuadorian waters calculated using three methods. Methods employed were Beverton and Holt [<a href="#B33-fishes-10-00005" class="html-bibr">33</a>] and Cushing [<a href="#B34-fishes-10-00005" class="html-bibr">34</a>]. The dotted line represents the optimal exploitation rate according to the maximum sustainable yield. The continuous line is the average value obtained for the species.</p>
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<p>Size–frequency distribution of <span class="html-italic">Pseudocarcharias kamoharai</span> and its reference population parameters. The black vertical line represents the optimal capture average size according to the maximum sustainable yield (<span class="html-italic">L<sub>opt</sub></span>), the grey line is the sexual maturity size of the population, and the dotted line is the asymptotic length of the individuals.</p>
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11 pages, 4970 KiB  
Article
Detecting Early Degradation of Wood Ultrastructure with Nonlinear Optical Imaging and Fluorescence Lifetime Analysis
by Alice Dal Fovo, Riccardo Cicchi, Claudia Gagliardi, Enrico Baria, Marco Fioravanti and Raffaella Fontana
Polymers 2024, 16(24), 3590; https://doi.org/10.3390/polym16243590 - 22 Dec 2024
Viewed by 907
Abstract
Understanding the deterioration processes in wooden artefacts is essential for accurately assessing their conservation status and developing effective preservation strategies. Advanced imaging techniques are currently being explored to study the impact of chemical changes on the structural and mechanical properties of wood. Nonlinear [...] Read more.
Understanding the deterioration processes in wooden artefacts is essential for accurately assessing their conservation status and developing effective preservation strategies. Advanced imaging techniques are currently being explored to study the impact of chemical changes on the structural and mechanical properties of wood. Nonlinear optical modalities, including second harmonic generation (SHG) and two-photon excited fluorescence (TPEF), combined with fluorescence lifetime imaging microscopy (FLIM), offer a promising non-destructive diagnostic method for evaluating lignocellulose-based materials. In this study, we employed a nonlinear multimodal approach to examine the effects of artificially induced delignification on samples of Norway spruce (Picea abies) and European beech (Fagus sylvatica) subjected to increasing treatment durations. The integration of SHG/TPEF imaging and multi-component fluorescence lifetime analysis enabled the detection of localized variations in nonlinear signals and τ-phase of key biopolymers within wood cell walls. This methodology provides a powerful tool for early detection of wood deterioration, facilitating proactive conservation efforts of wooden artefacts. Full article
(This article belongs to the Special Issue Advances in Applied Lignin Research)
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<p>Normalized averaged fluorescence spectra (λ<sub>ext</sub> = 445 nm) of spruce (<b>a</b>) and beech (<b>b</b>) and scatter plots of the peaks of the two main emission bands for spruce (<b>c</b>) and beech (<b>d</b>) at increasing treatment time.</p>
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<p>TPEF and SHG intensity images (300 × 300 µm<sup>2</sup>, 512 × 512 pixel) of spruce and beech samples, acquired before (DL = 0 h) and after the delignification treatment (DL = 48 h). The first and second columns show eight-bit grayscale images, representing the SHG and TPEF signal intensities as pixel brightness within the dynamic range of 0–255. The third column presents color-composite images where the SHG signal, primarily associated with cellulose, and the TPEF signal are displayed in green and red, respectively.</p>
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<p>FLIM analysis of the untreated spruce sample: color-coded lifetime image (25 × 25 µm<sup>2</sup>) with the mean lifetime values <math display="inline"><semantics> <mrow> <msub> <mi>τ</mi> <mrow> <mn>1</mn> <mo>−</mo> <mn>3</mn> </mrow> </msub> </mrow> </semantics></math> of the decay components (<b>a</b>), resulting from the triple-exponential fit of the experimental data; amplitude-weighted lifetime (<b>b</b>) showing how often the pixels with specific lifetime values occur in the matrix decay image (<b>a</b>).</p>
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<p>FLIM results on spruce and beech samples, acquired before (DL = 0 h) and after the delignification treatment (DL = 48 h): color-coded lifetime images (300 × 300 mm<sup>2</sup>, 512 × 512 pixel) and amplitude-weighted lifetime distributions.</p>
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<p>Scatter plots of average amplitudes (<b>a</b>–<b>c</b>) and lifetimes (<b>d</b>–<b>f</b>) for the three primary decay components, attributed to lignin, hemicellulose and cellulose, respectively, measured in spruce samples exposed to increasing hours of delignification. Error bars represent the standard deviation, and red lines indicate the exponential fit of the experimental data.</p>
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<p>Scatter plots of average amplitudes (<b>a</b>–<b>c</b>) and lifetimes (<b>d</b>) for the three primary decay components, attributed to lignin, hemicellulose and cellulose, respectively, measured in beech samples exposed to increasing hours of delignification. Error bars represent the standard deviation, and the red lines indicate the exponential (<math display="inline"><semantics> <mrow> <msub> <mi>a</mi> <mrow> <mn>1</mn> <mo>−</mo> <mn>3</mn> </mrow> </msub> </mrow> </semantics></math>) and linear (<math display="inline"><semantics> <mrow> <msub> <mi>τ</mi> <mrow> <mn>1</mn> <mo>−</mo> <mn>3</mn> </mrow> </msub> </mrow> </semantics></math>) fit of the experimental data.</p>
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12 pages, 3194 KiB  
Case Report
Imaging-Based Molecular Interaction Between Src and Lamin A/C Mechanosensitive Proteins in the Nucleus of Laminopathic Cells
by Stefania Petrini, Giulia Bagnato, Michela Piccione, Valentina D’Oria, Valentina Apollonio, Marco Cappa, Claudia Castiglioni, Filippo Maria Santorelli, Teresa Rizza, Rosalba Carrozzo, Enrico Silvio Bertini and Barbara Peruzzi
Int. J. Mol. Sci. 2024, 25(24), 13365; https://doi.org/10.3390/ijms252413365 - 13 Dec 2024
Viewed by 759
Abstract
Laminopathies represent a wide range of genetic disorders caused by mutations in gene-encoding proteins of the nuclear lamina. Altered nuclear mechanics have been associated with laminopathies, given the key role of nuclear lamins as mechanosensitive proteins involved in the mechanotransduction process. To shed [...] Read more.
Laminopathies represent a wide range of genetic disorders caused by mutations in gene-encoding proteins of the nuclear lamina. Altered nuclear mechanics have been associated with laminopathies, given the key role of nuclear lamins as mechanosensitive proteins involved in the mechanotransduction process. To shed light on the nuclear partners cooperating with altered lamins, we focused on Src tyrosine kinase, known to phosphorylate proteins of the nuclear lamina. Here, we demonstrated a tight relationship between lamin A/C and Src in skin fibroblasts from two laminopathic patients, assessed by advanced imaging-based microscopy techniques. With confocal laser scanning and Stimulated Emission Depletion (STED) microscopy, a statistically significant higher co-distribution between the two proteins was observed in patients’ fibroblasts. Furthermore, the time-domain fluorescence lifetime imaging microscopy, combined with Förster resonance energy transfer detection, demonstrated a decreased lifetime value of Src (as donor fluorophore) in the presence of lamin A/C (as acceptor dye) in double-stained fibroblast nuclei in both healthy cells and patients’ cells, thereby indicating a molecular interaction that resulted significantly higher in laminopathic cells. All these results demonstrate a molecular interaction between Src and lamin A/C in healthy fibroblasts and their aberrant interaction in laminopathic nuclei, thus creating the possibilities of new diagnostic and therapeutic approaches for patients. Full article
(This article belongs to the Special Issue Protein Signal Transduction in the Nucleus)
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<p>Confocal microscopy imaging of Src (in green) and lamin A/C (in red) in control and laminopathic fibroblasts. (<b>A</b>) Src immunofluorescence showed a punctate and diffuse distribution in the nuclear and cytoplasmic compartments, with a higher concentration in the nuclei, both in healthy cells and patients’ cells. Orange pixels showed the overlay of Src and Lamin A/C fluorescence in doubled-stained cells. Colocalization masks of double-stained cells (white pixels) showed the Src-lamin A/C co-distribution both at the nuclear envelope (arrows and arrowheads) and in the nucleoplasm. (<b>B</b>) Intensity line profiles of Src (green) and lamin A/C (red) across the focal central plane, as indicated by the white dotted line of representative nuclei in the overlay images. Scale bars: 10 μm for all images except insets (5 μm). (<b>C</b>) Src mean fluorescence intensity decreased in patients’ nuclei, significantly in Pt 1, compared to controls (* <span class="html-italic">p</span> &lt; 0.05).</p>
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<p>STED nanoscopy of Src and lamin A/C in nuclei from healthy and laminopathic fibroblasts. (<b>A</b>) In the healthy control nuclei, Src labeling (green) was thickened at the nuclear periphery, with a diffuse and dotted distribution in the nuclear matrix, whereas some anomalous aggregates were observed (arrows) in patients’ nuclei. Alterations in the structural organization of the lamin A/C (red) meshworks have been seen in several nuclei of the fibroblasts of patient 1 and patient 2 (arrowheads). Colocalization masks (yellow) showed the co-distribution of Src and lamin A/C at the nuclear rim in all samples and a higher concentration in the nucleoplasm of patients’ cells (high magnification of insets). Bars: 5 µm and 2 µm. (<b>B</b>) Mean values of the overlap coefficient quantified in STED images of double-stained fibroblast nuclei. (** <span class="html-italic">p</span> &lt; 0.01; * <span class="html-italic">p</span> &lt; 0.05).</p>
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<p>FLIM and FLIM-FRET microscopy of Src and lamin A/C in healthy and laminopathic fibroblast nuclei. (<b>A</b>) Fluorescence lifetime imaging of Src-AF488 donor in the absence (τ<sub>D</sub>, left panel) or in the presence (τ<sub>DA</sub>, right panel) of a lamin A/C-AF594 acceptor. Different τ values were visualized via color code lifetime scale bar (from 2.0 to 3.5 ns of range). (<b>B</b>) Src-AF488 mean lifetime values in the absence of the acceptor (τ<sub>D</sub>) showed a significant increase in laminopathic nuclei compared to controls (**** <span class="html-italic">p</span> &lt; 0.0001 in Pt 1; ** <span class="html-italic">p</span> &lt; 0.01 in Pt 2). (<b>C</b>) The statistical analysis of the Src-AF488 mean τ<sub>D</sub> values in the two specific ROIs revealed significant lifetime changes between controls and patients’ nuclei, both in the lamina and in the nuclear matrix regions (**** <span class="html-italic">p</span> &lt; 0.0001; * <span class="html-italic">p</span> &lt; 0.05). (<b>D</b>) Src-AF488 donor lifetime in the presence of the acceptor molecule (τ<sub>DA</sub>, amplitude weighted lifetime) was significantly decreased in all samples, with a greater extent in patients’ fibroblasts (**** <span class="html-italic">p</span> &lt; 0.0001). (<b>E</b>–<b>G</b>) Quantified FRET efficiency values (mean ± sem) of the Src-AF488 and lamin A/C-AF 594 pair obtained in all selected ROIs (<b>E</b>), at the nuclear rim (<b>F</b>) and in the nucleoplasm (<b>G</b>) in controls (gray dots), in Pt 1 (red dots) and Pt 2 (green dots) nuclei (**** <span class="html-italic">p</span> &lt; 0.0001; ** <span class="html-italic">p</span> &lt; 0.01; * <span class="html-italic">p</span> &lt; 0.05).</p>
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14 pages, 2990 KiB  
Article
Novel Optical Criteria and Mechanisms of Critical Decline in Liver Regenerative Potential
by Svetlana Rodimova, Vera Kozlova, Nikolai Bobrov, Dmitry Kozlov, Artem Mozherov, Vadim Elagin, Ilya Shchechkin, Dmitry Kuzmin, Alena Gavrina, Vladimir Zagainov, Elena Zagaynova and Daria Kuznetsova
Cells 2024, 13(23), 2015; https://doi.org/10.3390/cells13232015 - 5 Dec 2024
Viewed by 865
Abstract
The most effective method of treating tumors localized in the liver remains resection. However, in the presence of concomitant pathology, the regenerative potential of the liver is significantly reduced. To date, there is insufficient fundamental data on the mechanisms responsible for the disruption [...] Read more.
The most effective method of treating tumors localized in the liver remains resection. However, in the presence of concomitant pathology, the regenerative potential of the liver is significantly reduced. To date, there is insufficient fundamental data on the mechanisms responsible for the disruption of liver regeneration, and there is no effective method for assessing its regenerative potential. The most suitable model for these purposes is acute liver injury (ALI). Modern non-contrast methods of multiphoton microscopy with second harmonic generation and fluorescence lifetime imaging microscopy (FLIM) modes enable intravital evaluation of the metabolic status of the hepatocytes; therefore, this expands the possibilities for studying the processes occurring in cells during regeneration in the context of any pathologies. Full article
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<p>Road map of the steps in the experiment on liver regeneration with induced ALI.</p>
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<p>Analysis of the structural state of liver tissue in normal state and with ALI during induced regeneration after (<b>A</b>) 30% PH and (<b>B</b>) 70% PH. Fluorescence intensity images of NAD(P)H fluorescence and the second harmonic generation of collagen (green) in liver tissue. NAD(P)H fluorescence: excitation at 750 nm, detection range 455–500 nm; cell autofluorescence (red): excitation at 800 nm, detection range 433–660 nm; SHG (green): excitation at 800 nm, detection range 371–421 nm. Green arrows indicate collagen. The dotted line indicates a zone with reduced NAD(P)H fluorescence intensity. Scale bar: 50 μm; ×400.</p>
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<p>FLIM analysis of liver tissue with ALI during induced regeneration after 30% PH; (<b>A</b>) pseudo-coded FLIM images at different stages of liver regeneration in normal state and with ALI. (<b>B</b>) Boxplots reflecting the distribution of values of the fluorescence lifetime contributions of the bound forms of NADH and NADPH. Scale bar: 50 μm; ×400. *—statistically significant difference compared to normal liver (0 day). #—statistically significant differences compared to the corresponding time point for normal regeneration; <span class="html-italic">p</span>-value ≤ 0.05.</p>
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<p>FLIM analysis of liver tissue with ALI during induced regeneration after 70% PH; (<b>A</b>) pseudo-coded FLIM images at different stages of liver regeneration in normal state and with ALI. (<b>B</b>) Boxplots reflecting the distribution of values of the fluorescence lifetime contributions of the bound forms of NADH and NADPH. Scale bar: 50 μm; ×400. *—statistically significant difference compared to normal liver (0 day). #—statistically significant differences compared to the corresponding time point for normal regeneration; <span class="html-italic">p</span>-value ≤ 0.05.</p>
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<p>Analysis of liver weight recovery during regeneration in normal state and with induced ALI using 30% PH and 70% PH models. Each dot represents a measurement of the weight of one animal. Data are presented as mean ± standard deviation.</p>
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<p>Histological (<b>A</b>) and morphometric analysis (<b>B</b>,<b>C</b>) of liver tissue with ALI during induced regeneration after 30% PH and 70% PH, hematoxylin and eosin; black arrows indicate balloon dystrophy of hepatocytes; yellow arrows indicate vacuolated hepatocytes. *—statistically significant differences compared to the corresponding time point for normal regeneration; <span class="html-italic">p</span>-value ≤ 0.05. Scale bar: 50 μm; ×400.</p>
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<p>Biochemical analysis of the level of liver damage markers in the blood serum of rats during regeneration with concomitant ALI. The areas marked with a dotted line reflect the range of physiological values for each biochemical parameter under study.</p>
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<p>Analysis of changes in gene expression during normal regeneration and during regeneration with ALI. *—statistical differences for time points of normal regeneration from the corresponding time points of regeneration with ALI; <span class="html-italic">p</span>-value ≤ 0.05.</p>
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20 pages, 8833 KiB  
Article
Calcium Indicators with Fluorescence Lifetime-Based Signal Readout: A Structure–Function Study
by Tatiana R. Simonyan, Larisa A. Varfolomeeva, Anastasia V. Mamontova, Alexey A. Kotlobay, Andrey Y. Gorokhovatsky, Alexey M. Bogdanov and Konstantin M. Boyko
Int. J. Mol. Sci. 2024, 25(23), 12493; https://doi.org/10.3390/ijms252312493 - 21 Nov 2024
Viewed by 1428
Abstract
The calcium cation is a crucial signaling molecule involved in numerous cellular pathways. Beyond its role as a messenger or modulator in intracellular cascades, calcium’s function in excitable cells, including nerve impulse transmission, is remarkable. The central role of calcium in nervous activity [...] Read more.
The calcium cation is a crucial signaling molecule involved in numerous cellular pathways. Beyond its role as a messenger or modulator in intracellular cascades, calcium’s function in excitable cells, including nerve impulse transmission, is remarkable. The central role of calcium in nervous activity has driven the rapid development of fluorescent techniques for monitoring this cation in living cells. Specifically, genetically encoded calcium indicators (GECIs) are the most in-demand molecular tools in their class. In this work, we address two issues of calcium imaging by designing indicators based on the successful GCaMP6 backbone and the fluorescent protein BrUSLEE. The first indicator variant (GCaMP6s-BrUS), with a reduced, calcium-insensitive fluorescence lifetime, has potential in monitoring calcium dynamics with a high temporal resolution in combination with advanced microscopy techniques, such as light beads microscopy, where the fluorescence lifetime limits acquisition speed. Conversely, the second variant (GCaMP6s-BrUS-145), with a flexible, calcium-sensitive fluorescence lifetime, is relevant for static measurements, particularly for determining absolute calcium concentration values using fluorescence lifetime imaging microscopy (FLIM). To identify the structural determinants of calcium sensitivity in these indicator variants, we determine their spatial structures. A comparative structural analysis allowed the optimization of the GCaMP6s-BrUS construct, resulting in an indicator variant combining calcium-sensitive behavior in the time domain and enhanced molecular brightness. Our data may serve as a starting point for further engineering efforts towards improved GECI variants with fine-tuned fluorescence lifetimes. Full article
(This article belongs to the Collection Feature Papers in Molecular Biophysics)
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<p>Schematics showing the design of chimeric proteins used in the study. At the top, the spatial structure of GCaMP6 is shown, with the mutations required for the EGFP modification. In the center, there is a linear scheme of the GCaMP-type backbone. The numbering of amino acid positions corresponds to those of the unmodified proteins (EGFP and calmodulin). At the bottom (left and right), the modified variants, GCaMP6s-BrUS and GCaMP6s-BrUS-145, are displayed, with the introduced modifications displayed below them.</p>
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<p>Calcium sensitivity of purified GCaMP6s, GCaMP6s-BrUS, and GCaMP6s-BrUS-145 measured in the intensiometric mode. (<b>A</b>) The dependence of fluorescence intensity at 510 nm (λ<sub>ex</sub> = 475 nm) on calcium concentration, expressed as [Ca<sup>2+</sup>]<sub>free</sub> (see <a href="#app1-ijms-25-12493" class="html-app">Supplementary Table S1</a> for details on the correspondence between [Ca<sup>2+</sup>]<sub>free</sub> and [CaEGTA]). (<b>B</b>) Column histogram displaying the relative fluorescence intensity changes observed within the [Ca<sup>2+</sup>]<sub>free</sub> range of 0–39 μM (corresponds to the [CaEGTA] range of 0–10 mM). Standard errors of the mean (S.E.M.) are shown for each data point (<span class="html-italic">n</span> = 3).</p>
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<p>The graph describing the dependence of the amplitude-weighted mean fluorescence lifetime of indicator variants on calcium concentration ([CaEGTA] and [Ca<sup>2+</sup>]<sub>free</sub>; see <a href="#app1-ijms-25-12493" class="html-app">Supplementary Table S1</a> for details). λ<sub>ex</sub> = 450 nm, repetition rate is 20 MHz. Standard errors of the mean (S.E.M.) are shown for each data point (<span class="html-italic">n</span> = 3).</p>
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<p>Comparison of GCaMP6s-BrUS and GCaMP6s-BrUS-145 structures. (<b>A</b>,<b>B</b>) Superposition of GCaMP6s-BrUS and GCaMP6s-BrUS-145 (magenta) structures from two views. Color scheme for GCaMP6s-BrUS is the following: EFGP domain—green, CaM domain—blue, M13 helix—orange, and the linker 314–319—light gray. Chromophore and calcium ions are shown in light and dark gray color for GCaMP6s-BrUS and GCaMP6s-BrUS-145, respectively. Red arrows point to the shift of the linker 314–319 (<b>A</b>) and the C-lobe of the CaM domain (<b>B</b>). (<b>C</b>–<b>F</b>) Differences in the conformation of residues surrounding the chromophore. Panels (<b>C</b>,<b>E</b>) represent GCaMP6s-BrUS structure and (<b>D</b>,<b>F</b>) GCaMP6s-BrUS-145. Solvent molecules are shown as red spheres. Hydrogen bonds are depicted as dashed blue lines.</p>
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<p>Calcium sensitivity of GCaMP6s-BrUS-389K fluorescence. (<b>A</b>) The dependence of fluorescence intensity at 510 nm (λ<sub>ex</sub> = 475 nm) on calcium concentration, expressed as [Ca<sup>2+</sup>]<sub>free</sub>. (<b>B</b>) The graph describing the dependence of the amplitude-weighted mean fluorescence lifetime on calcium concentration ([CaEGTA] and [Ca<sup>2+</sup>]<sub>free</sub>). λ<sub>ex</sub> = 450 nm, repetition rate is 20 MHz. Standard errors of the mean (S.E.M.) are shown for each data point (<span class="html-italic">n</span> = 3).</p>
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<p>Calcium sensitivity of GCaMP6s-BrUS-389K/398G fluorescence. (<b>A</b>) The dependence of fluorescence intensity at 510 nm (λ<sub>ex</sub> = 475 nm) on calcium concentration, expressed as [Ca<sup>2+</sup>]<sub>free</sub>. (<b>B</b>) The graph describing the dependence of the amplitude-weighted mean fluorescence lifetime on calcium concentration ([CaEGTA] and [Ca<sup>2+</sup>]<sub>free</sub>). λ<sub>ex</sub> = 450 nm, repetition rate is 20 MHz. Standard errors of the mean (S.E.M.) are shown for each data point (<span class="html-italic">n</span> = 3).</p>
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19 pages, 6202 KiB  
Article
In Vitro Cell Model Investigation of Alpha-Synuclein Aggregate Morphology Using Spectroscopic Imaging
by Priyanka Swaminathan, Therése Klingstedt, Vasileios Theologidis, Hjalte Gram, Johan Larsson, Lars Hagen, Nina B. Liabakk, Odrun A. Gederaas, Per Hammarström, K. Peter R. Nilsson, Nathalie Van Den Berge and Mikael Lindgren
Int. J. Mol. Sci. 2024, 25(22), 12458; https://doi.org/10.3390/ijms252212458 - 20 Nov 2024
Cited by 1 | Viewed by 2919
Abstract
Recently, it has been hypothesized that alpha-synuclein protein strain morphology may be associated with clinical subtypes of alpha-synucleinopathies, like Parkinson’s disease and multiple system atrophy. However, direct evidence is lacking due to the caveat of conformation-specific characterization of protein strain morphology. Here we [...] Read more.
Recently, it has been hypothesized that alpha-synuclein protein strain morphology may be associated with clinical subtypes of alpha-synucleinopathies, like Parkinson’s disease and multiple system atrophy. However, direct evidence is lacking due to the caveat of conformation-specific characterization of protein strain morphology. Here we present a new cell model based in vitro method to explore various alpha-synuclein (αsyn) aggregate morphotypes. We performed a spectroscopic investigation of the HEK293 cell model, transfected with human wildtype-αsyn and A53T-αsyn variants, using the amyloid fibril-specific heptameric luminescent oligomeric thiophene h-FTAA. The spectral profile of h-FTAA binding to aggregates displayed a blue-shifted spectrum with a fluorescence decay time longer than in PBS, suggesting a hydrophobic binding site. In vitro spectroscopic binding characterization of h-FTAA with αsyn pre-formed fibrils suggested a binding dissociation constant Kd < 100 nM. The cells expressing the A53T-αsyn and human wildtype-αsyn were exposed to recombinant pre-formed fibrils of human αsyn. The ensuing intracellular aggregates were stained with h-FTAA followed by an evaluation of the spectral features and fluorescence lifetime of intracellular αsyn/h-FTAA, in order to characterize aggregate morphotypes. This study exemplifies the use of cell culture together with conformation-specific ligands to characterize strain morphology by investigating the spectral profiles and fluorescence lifetime of h-FTAA, based upon its binding to a certain αsyn aggregate. This study paves the way for toxicity studies of different αsyn strains in vitro and in vivo. Accurate differentiation of specific alpha-synucleinopathies is still limited to advanced disease stages. However, early subtype-specific diagnosis is of the utmost importance for prognosis and treatment response. The potential association of αsyn aggregates morphotypes detected in biopsies or fluids to disease phenotypes would allow for subtype-specific diagnosis in subclinical disease stage and potentially reveal new subtype-specific treatment targets. Notably, the method may be applied to the entire spectrum of neurodegenerative diseases by using a combination of conformation-specific ligands in a physicochemical environment together with other types of polymorphic amyloid variants and assess the conformation-specific features of various protein pathologies. Full article
(This article belongs to the Section Molecular Biology)
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<p>Emission spectra of h-FTAA binding to PFFs fixed at 1 µM concentration with varying concentrations of h-FTAA from (<b>A</b>) 1125 nM to 4500 nM to (<b>B</b>) 141 nM to 563 nM. The samples were excited at 450 nm and the emission was recorded in the range of 500–700 nm. Each spectrum was baseline corrected using h-FTAA emission in PBS only, respectively. The shaded region in each spectrum represents the standard deviation from triplicates of the varied concentrations of h-FTAA while keeping the concentration of PFFs fixed at 1 µM.</p>
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<p>Binding curve of PFFs (1 μM) vs. h-FTAA concentration (red squares). The blue triangles show the signal obtained from only h-FTAA in PBS. The excitation wavelength was 450 nm, and the spectra were collected as in <a href="#ijms-25-12458-f001" class="html-fig">Figure 1</a>. The dashed curves are simulations where the blue dashed line corresponds to 6% QY of h-FTAA in PBS (<a href="#ijms-25-12458-t001" class="html-table">Table 1</a>). Green dot-dashed: 1-site binding K<sub>d</sub> = 25 nM; QY 30%. Red dashed: two-site model, K<sub>d1</sub> = 100 nM; K<sub>d2</sub> = 300 nM. QY(h-FTAA/PFF-site1) 40%; QY(h-FTAA/PFF-site2) 20%. For details of the two-site model, see [<a href="#B32-ijms-25-12458" class="html-bibr">32</a>].</p>
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<p>Hyperspectral imaging and fluorescence lifetime measurements of PFFs stained with 500 nM h-FTAA. (<b>A</b>) Representative fluorescence image and (<b>B</b>) False-color coded FLIM image of PFFs stained with h-FTAA. The sample was excited at 475 nm and the photons were collected in the 500–700 nm range. The color bar to the right represents the lifetime ranging from 0 ns to 2 ns. (<b>C</b>) Spectral analysis of h-FTAA when it is bound to PFFs, showing emission maxima at approximately 540 nm and 580 nm. The five ROIs (red) used to record the emission spectra are shown in (<b>B</b>). (<b>D</b>) Fluorescence decay time distribution recorded from the FLIM image using the same ROIs (red) that were selected for the spectral analysis in (<b>C</b>). The shaded regions in the plots represent the standard deviation.</p>
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<p>Endogenous αsyn expressed in HEK293 cells after transfection with 4 μg human A53T-αsyn or WT-αsyn. (<b>A</b>) Western blot showing αsyn protein bands at approximately 14 kDa in A53T-αsyn and WT-αsyn HEK293 cells which were probed with mouse anti-αsyn antibody Syn211. Representative immunofluorescence images of (<b>B</b>) A53T-αsyn, (<b>C</b>) WT-αsyn HEK293 cells showing localization of αsyn in cytosol, and (<b>D</b>) Untransfected HEK293 cells showing absence of αsyn, when labeled with mouse anti-αsyn antibody Syn211. Scale bar represents 10 µm.</p>
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<p>Representative fluorescence images of HEK293 cells expressing (<b>A</b>) A53T-αsyn or (<b>B</b>) WT-αsyn, seeded with 500 nM human-αsyn PFFs and stained with 1 μM h-FTAA (green) and 5 µM DRAQ5 (red). (<b>C</b>) Untransfected HEK293 cells were also exposed to PFFs, showing minimal fluorescence from h-FTAA. Scale bar represents 10 μm.</p>
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<p>Representative spectral analysis and lifetime distributions of h-FTAA binding to aggregates in A53T-αsyn-HEK293 and WT-αsyn-HEK293 cells. The samples were excited at 475 nm. (<b>A</b>) Emission spectra and (<b>B</b>) lifetime distributions of h-FTAA binding to aggregates in A53T-αsyn (red) and WT-αsyn-HEK293 (green) cells. Shaded areas correspond to the standard deviation of 5 ROIs.</p>
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<p>Representative differential interference contrast (DIC) and confocal microscopy images showing h-FTAA-stained (green), pS129-probed αsyn aggregates (red) in (<b>A</b>) A53T-αsyn-HEK293 cells and (<b>B</b>) WT-αsyn-HEK293 cells. The samples were excited at 475 nm and 650 nm, respectively. (<b>C</b>) Untransfected HEK293 cells, also seeded with PFFs, show no fluorescence from h-FTAA or the anti-αsyn pS129 antibody, indicating absence of pS129-positive αsyn aggregates. Scale bar represents 25 µm.</p>
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<p>Representative spectral analysis and lifetime distributions of h-FTAA-stained, pS129-labeled aggregates in A53T-αsyn-HEK293 and WT-αsyn-HEK293 cells. The samples were excited at 475 nm and 650 nm for h-FTAA and Alexa Fluor 647, respectively. (<b>A</b>) Emission spectra and (<b>B</b>) life-time distributions for h-FTAA-stained, pS129-labeled aggregates in A53T-αsyn-HEK293 and WT-αsyn-HEK293 cells. Shaded areas correspond to the standard deviation of 5 ROIs.</p>
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12 pages, 5537 KiB  
Article
Accompanying Hemoglobin Polymerization in Red Blood Cells in Patients with Sickle Cell Disease Using Fluorescence Lifetime Imaging
by Fernanda Aparecida Borges da Silva, João Batista Florindo, Amilcar Castro de Mattos, Fernando Ferreira Costa, Irene Lorand-Metze and Konradin Metze
Int. J. Mol. Sci. 2024, 25(22), 12290; https://doi.org/10.3390/ijms252212290 - 15 Nov 2024
Viewed by 1034
Abstract
In recent studies, it has been shown that fluorescence lifetime imaging (FLIM) may reveal intracellular structural details in unstained cytological preparations that are not revealed by standard staining procedures. The aim of our investigation was to examine whether FLIM images could reveal areas [...] Read more.
In recent studies, it has been shown that fluorescence lifetime imaging (FLIM) may reveal intracellular structural details in unstained cytological preparations that are not revealed by standard staining procedures. The aim of our investigation was to examine whether FLIM images could reveal areas suggestive of polymerization in red blood cells (RBCs) of sickle cell disease (SCD) patients. We examined label-free blood films using auto-fluorescence FLIM images of 45 SCD patients and compared the results with those of 27 control persons without hematological disease. All control RBCs revealed homogeneous cytoplasm without any foci. Rounded non-sickled RBCs in SCD showed between zero and three small intensively fluorescent dots with higher lifetime values. In sickled RBCs, we found additionally larger irregularly shaped intensively fluorescent areas with increased FLIM values. These areas were interpreted as equivalent to polymerized hemoglobin. The rounded, non-sickled RBCs of SCD patients with homogeneous cytoplasm were not different from those of the erythrocytes of control patients in light microscopy. Yet, variables from the local binary pattern-transformed matrix of the FLIM values per pixel showed significant differences between non-sickled RBCs and those of control cells. In a linear discriminant analysis, using local binary pattern-transformed texture features (mean and entropy) of the erythrocyte cytoplasm of normal appearing cells, the final model could distinguish between SCD patients and control persons with an accuracy of 84.7% of the patients. When the classification was based on the examination of a single rounded erythrocyte, an accuracy of 68.5% was achieved. Employing the Linear Discriminant Analysis classifier method for machine learning, the accuracy was 68.1%. We believe that our study shows that FLIM is able to disclose the topography of the intracellular polymerization process of hemoglobin in sickle cell disease and that the images are compatible with the theory of the two-step nucleation. Furthermore, we think that the presented technique may be an interesting tool for the investigation of therapeutic inhibition of polymerization. Full article
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<p>Image of a peripheral blood film of a control case with several normal RBCs. Upper left: auto-fluorescence picture. Upper middle: fluorescence lifetime image: the blue color corresponds to the lifetime of hemoglobin. Surrounding plasma in green/yellow color corresponding to a higher lifetime. A cursor is placed on a RBC (right inferior corner). Upper right: histogram of the lifetime distribution of the image (pseudo-colors according to the rainbow spectrum). Blue represents the shortest lifetime and red is the longest. The histogram shows that hemoglobin has a short lifetime. Below is the fluorescence lifetime decay curve of the selected spot in the image. Every dot represents a single photon.</p>
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<p>Upper left: autofluorescence and FLIM images of a patient with homozygous SS hemoglobinopathy. Two normal-shaped and one sickled RBC. Each of the normal looking ones shows one highly fluorescent dot. The sickled RBC has areas with a higher fluorescence suggestive of polymerization. The histogram on the right side represents the lifetime of the region where the cursor is placed. Lower right is the decay curve of the selected region of interest.</p>
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<p>RBCs from a blood smear of a patient with SC hemoglobinopathy. Left: auto-fluorescence and right FLIM image. In the center, a sickled cell with an irregular heterogeneous area of enhanced fluorescence revealing a higher lifetime value in the FLIM compared to the surrounding cytoplasm. Some of the non-sickled RBCs show highly fluorescent dots.</p>
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<p>RBCs from a blood smear of S beta-thalassemia hemoglobinopathy. Three entire sickled cells with irregular, sometimes heterogeneous areas with enhanced fluorescence revealing higher lifetime values compared to the surrounding cytoplasm. Some of the non-sickled RBCs show highly fluorescent dots.</p>
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<p>Distribution of non-sickled cells in patients with SCD according to the sub-types: SS in black, SC in green, and S thalassemia in orange. There were no significant differences among the different sub-types of SCD.</p>
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<p>Dot plot showing the distribution of LBP mean (Y axis) and LBP entropy (X axis) to show the distribution of each cell in the control group (blue), and SCD: non-sickled cells are in green and sickled cells are in orange. Both parameters were able to discriminate between normal and SCD in 84.7% of the cases.</p>
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16 pages, 5439 KiB  
Article
Unraveling Microviscosity Changes Induced in Cancer Cells by Photodynamic Therapy with Targeted Genetically Encoded Photosensitizer
by Liubov E. Shimolina, Aleksandra E. Khlynova, Vadim V. Elagin, Pavel A. Bureev, Petr S. Sherin, Marina K. Kuimova and Marina V. Shirmanova
Biomedicines 2024, 12(11), 2550; https://doi.org/10.3390/biomedicines12112550 - 8 Nov 2024
Viewed by 1077
Abstract
Background: Despite the fundamental importance of cell membrane microviscosity, changes in this biophysical parameter of membranes during photodynamic therapy (PDT) have not been fully understood. Methods: In this work, changes in the microviscosity of membranes of live HeLa Kyoto tumor cells were studied [...] Read more.
Background: Despite the fundamental importance of cell membrane microviscosity, changes in this biophysical parameter of membranes during photodynamic therapy (PDT) have not been fully understood. Methods: In this work, changes in the microviscosity of membranes of live HeLa Kyoto tumor cells were studied during PDT with KillerRed, a genetically encoded photosensitizer, in different cellular localizations. Membrane microviscosity was visualized using fluorescence lifetime imaging microscopy (FLIM) with a viscosity-sensitive BODIPY2 rotor. Results: Depending on the localization of the phototoxic protein, different effects on membrane microviscosity were observed. With nuclear localization of KillerRed, a gradual decrease in microviscosity was detected throughout the entire observation period, while for membrane localization of KillerRed, a dramatic increase in microviscosity was observed in the first minutes after PDT, and then a significant decrease at later stages of monitoring. The obtained data on cell monolayers are in good agreement with the data obtained for 3D tumor spheroids. Conclusions: These results indicate the involvement of membrane microviscosity in the response of tumor cells to PDT, which strongly depends on the localization of reactive oxygen species attack via targeting of a genetically encoded photosensitizer. Full article
(This article belongs to the Special Issue Photodynamic Therapy (3rd Edition))
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Figure 1
<p>The schematic mechanism of action of KillerRed protein as a genetically encoded photosensitizer for PDT. The gene encoding KillerRed is incorporated in cancer cells (HeLa Kyoto) through lentiviral transduction to ensure the expression of the protein in a targeted compartment—the cell nucleus (KillerRed-H2B) or the plasma membrane (KillerRed-PM). PDT with KillerRed results in the formation of ROS via the type I photoreaction, which leads to oxidative damage in the targeting site and other compartments.</p>
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<p>The molecular structure of molecular rotor BODIPY2.</p>
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<p>(<b>A</b>) Localization of the genetically encoded photosensitizer KillerRed in the nucleus and plasma membrane of HeLa cells and of the fluorescent molecular rotor in the plasma membrane. The scale bar is 40 µm, applicable to all images. (<b>B</b>) Photobleaching of KillerRed after PDT. Quantification of the fluorescence intensity in the cells after PDT. Means ± SD, <span class="html-italic">n</span> = 50 cells. The scale bar is 40 µm, applicable to all images. H2B: cells with nuclear localization of KillerRed, PM: cells with membrane localization of KillerRed.</p>
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<p>Cell viability and ROS analysis in cells after PDT with genetically encoded KillerRed protein. (<b>A</b>) Live (green)/dead (red) cells (LD) and ROS assay fluorescence images 10 min and 1 h after PDT. The bar is 40 µm, applicable to all images. (<b>B</b>) Quantitative analysis of dead cells in control and treated cell populations, %. (<b>C</b>) Viability of control and treated cells in 24 h after PDT, determined using the MTT assay. (<b>D</b>) Quantitative analysis of ROS in control and treated cell populations. Fluorescence intensity of DCFH-DA is shown as means ± SD. CNT: control with different localization of KillerRed. H2B: cells with nuclear localization of KillerRed. PM: cells with membrane localization of KillerRed. * <span class="html-italic">p</span> &lt; 0.05 with control; # <span class="html-italic">p</span> &lt; 0.05 with KillerRed-H2B.</p>
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<p>Analysis of products of lipid peroxidation: diene (DC) and triene (TC) conjugates and the Schiff bases (SB) for nuclear (<b>A</b>,<b>B</b>) and membrane localizations (<b>C</b>,<b>D</b>) of KillerRed. Means ± SD, <span class="html-italic">n</span> = 5 measurements. * Statistically significant differences in untreated control with KillerRed (<span class="html-italic">p</span> &lt; 0.05). CNT H2B: control with nuclear localization of KillerRed, CNT PM: control with membrane localization of KillerRed.</p>
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<p>Plasma membrane viscosity in HeLa Kyoto cells with KillerRed during PDT. (<b>A</b>) Representative FLIM images of cells with both localizations of KillerRed. The bar is 40 µm, applicable to all images. (<b>B</b>) Quantification of viscosity of plasma membranes in HeLa Kyoto cells. Means ± SD, <span class="html-italic">n</span> = 100 cells for each time point. * <span class="html-italic">p</span> &lt; 0.05 with control; # <span class="html-italic">p</span> &lt; 0.05 with KillerRed-H2B. CNT KR: control with different localization of KillerRed. H2B: cells with nuclear localization of KillerRed. PM: cells with membrane localization of KillerRed.</p>
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<p>Plasma membrane microviscosity in HeLa tumor spheroids after PDT with KillerRed localized in the nuclei (H2B) or within the plasma membrane (PM). (<b>A</b>) Schematic representation of the spheroid area (shown by the yellow square) imaged by FLIM. The spheroid had adhered to the glass bottom, and the images were acquired from a depth of ~30 μm. Higher-magnification image of the molecular rotor distribution in spheroid cell membranes indicated by the red squares. The scale bar is 80 μm. (<b>B</b>) FLIM images and live/dead (LD) assay of control and treated cells in spheroids. Bar = 80 μm. (<b>C</b>) Morphology of control and treated spheroids. The scale bar is 80 μm. (<b>D</b>) Quantification of membrane microviscosity of spheroid cells after PDT. Means ± SD, <span class="html-italic">n</span> = 4 spheroids, 60 cells in each. (<b>E</b>) Quantitative analysis of dead cells in control and treated cell populations, %. * <span class="html-italic">p</span> &lt; 0.05 with control; # <span class="html-italic">p</span> &lt; 0.05 with KillerRed-H2B. CNT KR: control with different localization of KillerRed. H2B: cells with nuclear localization of KillerRed. PM: cells with membrane localization of KillerRed.</p>
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15 pages, 4456 KiB  
Article
Interaction Dynamics of Plant-Specific Insert Domains from Cynara cardunculus: A Study of Homo- and Heterodimer Formation
by Miguel Sampaio, Sofia Santos, Ana Marta Jesus, José Pissarra, Gian Pietro Di Sansebastiano, Jonas Alvim and Cláudia Pereira
Molecules 2024, 29(21), 5139; https://doi.org/10.3390/molecules29215139 - 30 Oct 2024
Viewed by 869
Abstract
Plant aspartic proteinases (APs) from Cynara cardunculus feature unique plant-specific insert (PSI) domains, which serve as essential vacuolar sorting determinants, mediating the transport of proteins to the vacuole. Although their role in vacuolar trafficking is well established, the exact molecular mechanisms that regulate [...] Read more.
Plant aspartic proteinases (APs) from Cynara cardunculus feature unique plant-specific insert (PSI) domains, which serve as essential vacuolar sorting determinants, mediating the transport of proteins to the vacuole. Although their role in vacuolar trafficking is well established, the exact molecular mechanisms that regulate PSI interactions and functions remain largely unknown. This study explores the ability of PSI A and PSI B to form homo- and heterodimers using a combination of pull-down assays, the mating-based split-ubiquitin system (mbSUS), and FRET-FLIM analyses. Pull-down assays provided preliminary evidence of potential PSI homo- and heterodimer formation. This was conclusively validated by the more robust in vivo mbSUS and FRET-FLIM assays, which clearly demonstrated the formation of both homo- and heterodimers between PSI A and PSI B within cellular environments. These findings suggest that PSI dimerization is related to their broader functional role, particularly in protein trafficking. Results open new avenues for future research to explore the full extent of PSI dimerization and its implications in plant cellular processes. Full article
(This article belongs to the Section Molecular Structure)
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Graphical abstract

Graphical abstract
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<p>(<b>A</b>) Schematic representation of PSI-tagged versions used in pull-down assays. SDS-PAGE analysis of PSI–PSI interactions by pull-down assay at pH 6.8 (<b>B</b>,<b>C</b>) and 7.4 (<b>D</b>,<b>E</b>). (<b>B</b>(<b>a</b>),<b>C,D</b>(<b>a</b>) and <b>E</b>) Inputs and pull-down reactions were analyzed on a silver-stained gel. Each pull-down lane was loaded with 15 μL of pull-down reaction and input lanes were loaded with 1/3 of the amount of purified protein added to each reaction. (<b>B</b>)(<b>b</b>)–(<b>D</b>)(<b>b</b>) Western blot analysis to evaluate the presence of FLAG-tagged PSIs in the pull-down reactions. MW: Molecular Weight (PageRuler<sup>TM</sup> Prestained Protein Ladder, Thermo Scientific, Waltham, MA, USA). Red, green, and blue arrows represent GST-PSIA/PSIB-6xHis, FLAG-PSI A-6xHis, and FLAG-PSIB-6xhis, respectively.</p>
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<p>Split ubiquitin yeast two-hybrid assay. (<b>A</b>) Illustrations represent the bait and prey structures. The bait protein is fused to a typical GPI anchor [<a href="#B22-molecules-29-05139" class="html-bibr">22</a>]. (<b>B</b>) Yeast mating-based split-ubiquitin assay for interaction, including negative control (NubG) and positive control (NubI). Yeast diploids dropped at 1:10 and 1:100 dilutions spotted (<b>left</b> to <b>right</b>) on complete synthetic medium without Trp, Leu, Ura, and Met (CSM-LTUM) to verify mating; on CSM without Trp, Leu, Ura, Ade, His, and Met (CSM-LTUMAH) to verify adenine- and histidine-independent growth; and with Met additions to suppress bait expression.</p>
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<p>FRET-FLIM interaction assay. (<b>A</b>) Schematic representation of the fluorescent protein fusions performed in this study. Blue, yellow, green, and red rectangles represent SP-PSIA, SP-PSIB, green fluorescent protein (GFP), and red fluorescent protein (mCherry), respectively. (<b>B</b>) Mean lifetime graphic representation of PSI A—PSIA/B fluorescent protein pairs. Asterisks represent statistically significant differences in mean fluorescence lifetime with an α threshold of 0.05 and a 95% confidence interval (***, <span class="html-italic">p</span> &lt; 0.0002; ****, <span class="html-italic">p</span> &lt; 0.0001). (<b>C</b>) Subcellular localization of PSI A—PSIA/B fluorescent protein pairs. (<b>D</b>) Mean lifetime graphic representation of PSI B—PSI A/B fluorescent protein pairs. Asterisks represent statistically significant differences in mean fluorescence lifetime with an α threshold of 0.05 and a 95% confidence interval (****, <span class="html-italic">p</span> &lt; 0.0001). (<b>E</b>) Subcellular localization of PSI B—PSIA/B fluorescent protein pairs. SP—signal peptide.</p>
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<p>Bioinformatic analysis of the cardoon PSI A and PSI B amino acidic sequence. (<b>A</b>) Identification of conserved regions between PSI A and PSI B. Analysis performed with NetPhos 3.1 webtool (<a href="https://services.healthtech.dtu.dk/services/NetPhos-3.1/" target="_blank">https://services.healthtech.dtu.dk/services/NetPhos-3.1/</a>, accessed on 21 January 2024). Yellow zones represent conserved regions between PSI A and B while the red asterisk (*) represents a glycosylation site in PSI B. (<b>B</b>) Prediction of phosphorylation sites in both PSIs. Produced with Jalview webtool (<a href="https://www.jalview.org" target="_blank">https://www.jalview.org</a>, accessed on 21 January 2024). (<b>C</b>) Analysis of the hydrophilic potential of PSI A and PSI B amino acid sequence. Produced with Jalview webtool (<a href="https://www.jalview.org/" target="_blank">https://www.jalview.org/</a>, accessed on 21 January 2024) (<b>D</b>) Lipid binding potential prediction of amino acid regions in cardoon PSI A and PSI B. Analysis done with DisoLipPred webtool (<a href="http://biomine.cs.vcu.edu/servers/DisoLipPred/" target="_blank">http://biomine.cs.vcu.edu/servers/DisoLipPred/</a>, accessed on 21 January 2024). (<b>E</b>) Tertiary structure prediction of PSI A and PSI B. Double-edged red arrow is used to show that PSI A possesses a clustered tertiary structure while PSI B is a bit wider. Produced with AlphaFold webtool (<a href="https://alphafold.ebi.ac.uk/" target="_blank">https://alphafold.ebi.ac.uk/</a>, accessed on 21 January 2024). Dashed lines represent the threshold value for putative lipid interaction detected by the software. In all figures, the yellow square represents an uncharacterized but conserved loop region found in both PSIs that has potential for lipid interaction and therefore may interact with membranes.</p>
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