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Erythrocyte fragility

Erythrocyte fragility refers to the susceptibility of red blood cells (erythrocytes) to hemolysis under osmotic or mechanical stress, reflecting the integrity of the cell membrane, cytoskeleton, and surface area-to-volume ratio.^[1] Osmotic fragility assesses resistance to hypotonic solutions, where normal biconcave erythrocytes can swell by up to approximately 70% before rupturing, while cells with altered morphology, such as spherocytes, show increased fragility.^[2] Mechanical fragility evaluates hemolysis under physical forces, such as shear stress in circulation or during blood handling, and is relevant to conditions affecting membrane deformability. The osmotic fragility test, introduced by Parpart et al. in 1947, is a traditional method for quantifying osmotic fragility, with modern techniques including flow cytometry.^[1] Mechanical fragility is measured using assays like rotational viscometry or microfluidic devices to simulate circulatory stresses. Clinically, fragility tests aid in diagnosing hemolytic anemias like hereditary spherocytosis (increased osmotic fragility) or evaluating stored blood quality (mechanical fragility), though results must be interpreted alongside other diagnostics.^[3]

Overview

Definition and physiological role

Erythrocyte fragility refers to the susceptibility of red blood cells (erythrocytes) to hemolysis when exposed to osmotic or mechanical stresses, reflecting the integrity of their membrane and cytoskeletal structure beyond the normal 120-day lifespan in circulation.^[4] This property is not pathological in itself but represents a baseline measure of cellular resilience, where excessive fragility leads to premature cell destruction and hemolytic disorders, while insufficient fragility is rare and less clinically relevant.^[5] In physiological terms, balanced erythrocyte fragility plays a critical role in enabling red blood cells to navigate the microcirculation—such as squeezing through capillaries narrower than their diameter—without lysing prematurely, thereby sustaining efficient oxygen delivery to tissues.^[6] The biconcave disc shape of erythrocytes optimizes their surface area-to-volume ratio, allowing up to a 70% increase in volume under hypotonic conditions or reversible deformation under shear stress before reaching the lysis threshold, which supports unobstructed blood flow and gas exchange.^[4] This adaptability is essential for maintaining vascular homeostasis, as compromised fragility could disrupt perfusion in low-oxygen environments or high-shear areas like the spleen.^[7] The structural prerequisites for this fragility balance include the erythrocyte's plasma membrane, a lipid bilayer rich in phospholipids and cholesterol that provides fluidity, anchored to an underlying cytoskeleton composed primarily of spectrin, actin, and protein 4.1, which imparts tensile strength and elasticity.^[8] Encapsulated within this framework is hemoglobin, the oxygen-carrying protein that constitutes about 95% of the cell's dry weight, but the membrane-cytoskeleton complex is paramount for withstanding circulatory stresses without compromising intracellular contents.^[9] These elements collectively ensure that erythrocytes remain intact during their journey, contributing to overall cardiovascular efficiency and tissue oxygenation.^[10]

Historical development

The concept of erythrocyte fragility emerged from 19th-century observations of red blood cell (RBC) behavior in hypotonic solutions, where early physiologists noted cellular swelling and lysis due to osmotic stress. George Gulliver's detailed measurements of mammalian blood corpuscles in the 1840s provided foundational insights into RBC morphology and volume changes under varying conditions, laying groundwork for understanding osmotic effects on cell integrity. By the early 20th century, Maurice Chauffard in 1907 reported increased osmotic fragility in patients with hereditary spherocytosis, marking the first clinical correlation between altered RBC resistance to hypotonic solutions and hemolytic anemia.^[11]^[12]^[13] In the 1920s and 1930s, standardized fragility tests gained traction for diagnosing hemolytic anemias, with methods involving serial dilutions of saline to quantify hemolysis thresholds proving valuable in identifying membrane defects. Thomas Hale Ham's work in the 1940s further advanced the field by demonstrating heightened osmotic fragility in paroxysmal nocturnal hemoglobinuria (PNH), complementing his acidified serum lysis test and highlighting acquired membrane vulnerabilities in hemolytic disorders. These developments shifted focus from mere observation to quantitative assessment, enabling broader clinical application in differentiating congenital and acquired anemias.^[12]^[14]^[15] Post-1950s research integrated fragility studies with membrane biochemistry, revealing cytoskeletal components' roles in RBC stability. The discovery of spectrin in 1968 by Marchesi and Steers, followed by 1970s investigations elucidating its function in the membrane skeleton, explained how defects in spectrin networks contribute to increased fragility in hereditary disorders. This era's biochemical insights transformed fragility from a phenomenological test into a window on molecular pathology.^[16]^[17] In the 21st century, refinements such as flow cytometry-based osmotic fragility assays, introduced around 2008, offered higher sensitivity and objectivity by analyzing light scatter in hypotonic gradients, improving detection in subtle cases. Ektacytometry, advanced since the 1970s but optimized in recent decades, quantifies deformability under shear and osmotic stress, providing precise fragility metrics. Recent 2020s studies have applied these techniques to sickle cell disease variants, linking elevated fragility to hemolysis rates and vaso-occlusive events, as seen in analyses of RBC deformability biomarkers.^[18]^[19]^[20]

Osmotic fragility

Underlying mechanisms

Osmotic fragility refers to the susceptibility of erythrocytes to hemolysis in hypotonic solutions, primarily due to water influx that causes cell swelling and eventual membrane rupture. In hypotonic environments, water enters the cell via osmosis through aquaporin channels, increasing intracellular volume while the semi-permeable lipid bilayer resists expansion. The biconcave disc shape of normal erythrocytes provides a high surface area-to-volume ratio, allowing swelling up to approximately 70% before lysis occurs, as the excess membrane accommodates volume changes without immediate rupture.^[1] This fragility is influenced by membrane integrity and composition, including the spectrin-based cytoskeleton that maintains structural stability. Defects in membrane proteins, such as ankyrin or band 3 in hereditary spherocytosis, lead to spherocyte formation with reduced surface area-to-volume ratio, causing earlier lysis at higher saline concentrations (e.g., hemolysis starting at 0.6-0.7% NaCl vs. 0.45-0.5% in normals). Conversely, conditions like thalassemia produce target cells with excess membrane surface area, conferring resistance to osmotic stress and delaying hemolysis until lower concentrations (e.g., below 0.3% NaCl). Additional factors include intracellular ion balances, where increased sodium or calcium can alter membrane rigidity and fragility.^[1]^[2]

Measurement techniques

The primary method for assessing osmotic fragility is the osmotic fragility test (OFT), which involves suspending fresh EDTA-anticoagulated whole blood in a series of hypotonic saline solutions (typically 0.30% to 0.90% NaCl) and quantifying hemolysis by measuring released hemoglobin via spectrophotometry at 540 nm. In the standard unincubated test, hemolysis begins around 0.45-0.50% NaCl and completes by 0.30-0.35% NaCl for normal erythrocytes, with the median hemolytic concentration (MHC50) at 0.40-0.45% NaCl. An incubated variant, where samples are held at 37°C for 24 hours to mimic in vivo metabolic stress and sodium accumulation, increases sensitivity, shifting the curve rightward (e.g., hemolysis starting at 0.60% NaCl). A control sample from a healthy individual is required for comparison, as results are reported as percentage hemolysis relative to the control.^[1]^[21] Modern alternatives include flow cytometry-based osmotic fragility tests, which use fluorescent dyes to detect lysed cells or measure forward scatter changes in hypotonic buffers, offering higher precision and reduced sample volume. Automated analyzers, such as those employing laser diffraction or impedance, provide deformability indices under osmotic stress but are less specific for fragility. Limitations include variability from sample handling (e.g., temperature affecting membrane integrity by 10-15%), reticulocytosis falsely decreasing fragility, and the need for fresh blood (results invalid after 48 hours). As of 2025, flow cytometric methods are increasingly adopted for their objectivity, though traditional OFT remains standard due to accessibility.^[21]^[22]

Clinical applications

Osmotic fragility testing is primarily used to diagnose hereditary spherocytosis (HS), an inherited hemolytic anemia caused by red cell membrane defects, where increased fragility (e.g., >50% hemolysis at 0.60 g/dL NaCl in incubated samples) supports diagnosis when combined with peripheral blood smear showing spherocytes and family history. It detects mild HS cases missed by morphology alone, guiding decisions like splenectomy to reduce hemolysis. The test may be normal in 10-20% of mild HS due to compensated states or mosaicism.^[3]^[21] Decreased osmotic fragility is characteristic of thalassemia and iron deficiency anemia, where target cells resist lysis (e.g., <10% hemolysis at 0.30% NaCl), aiding differentiation from other microcytic anemias. Increased fragility also occurs in acquired conditions like autoimmune hemolytic anemia, G6PD deficiency, or post-splenectomy states, while normal or decreased fragility appears in sickle cell disease or liver disease. The test is not standalone; it must correlate with eosin-5-maleimide (EMA) flow cytometry or genetic testing for confirmation, as false positives arise from sample artifacts or concurrent infections. As of November 2025, guidelines from bodies like the American Society of Hematology recommend OFT as a supportive tool in HS evaluation, with emerging flow-based assays improving specificity in pediatric and atypical cases.^[1]^[3]

Mechanical fragility

Underlying mechanisms

Erythrocytes, or red blood cells (RBCs), experience mechanical fragility primarily due to shear stresses encountered during circulation, which induce membrane stretching and deformation. In the microvasculature and larger vessels, fluid shear forces act on the RBC membrane, causing it to extend and alter shape to navigate narrow passages. The viscoelastic properties of the underlying spectrin-actin cytoskeleton provide resistance to these deformations, maintaining structural integrity through a network of spectrin tetramers cross-linked by actin junctions and anchored to the lipid bilayer via ankyrin and band 3 proteins. This skeletal framework enables reversible shape changes, such as the biconcave disc transforming into an ellipsoid under moderate shear, preventing immediate rupture.^[23]^[24] Under excessive shear, failure occurs through the formation of pores in the membrane, leading to hemolysis. High shear rates exceeding 1000 s⁻¹, as found in certain microvascular regions or pathological flows, stretch the membrane beyond its elastic limit, initiating nanopores (10–40 nm in diameter) in areas of localized strain. These pores allow hemoglobin leakage, with the spectrin network limiting pore expansion to approximately 75 nm before cytoskeleton rupture. In vitro models describe the hemolysis rate using a power-law relationship, where the index of hemolysis (IH) is proportional to τ^α, with τ as shear stress and α ≈ 2.4–3 from experimental data on laminar flows; exposure time further modulates this via an exponent β ≈ 0.8, emphasizing the cumulative damage from prolonged stress.^[25]^[26] Specific mechanical stressors, such as impacts from prosthetic heart valves or artificial circulatory devices, exacerbate fragility by generating peak shear stresses up to 1000 Pa, far beyond physiological levels. These devices induce transient high-shear zones that disrupt membrane-cytoskeleton linkages without involving volume changes, unlike osmotic stress; instead, the focus is on impaired shape recovery and increased pore susceptibility post-deformation. In contrast to osmotic mechanisms, mechanical fragility emphasizes solid-force induced lysis centered on cytoskeletal resilience rather than fluid-driven swelling.^[27]^[28]

Measurement techniques

Mechanical fragility of erythrocytes is assessed through in vitro techniques that simulate circulatory shear stresses, focusing on hemolysis propensity and cell deformation under controlled mechanical loads. Standard assays include microfluidic shear stress assays, which employ microfluidic channels to apply precise shear forces, mimicking microcirculatory conditions and quantifying cell passage or lysis rates. For instance, micropillar-based microfluidic devices measure erythrocyte transit through narrow constrictions under shear rates up to 1000 s⁻¹, revealing fragility by tracking deformation and fragmentation. Another common approach is the hemolysis index determination following exposure to rotating shear devices, such as cone-and-plate viscometers or impeller systems, where erythrocytes are subjected to high shear (e.g., 500–2000 s⁻¹) for defined durations, with the index calculated as the percentage of free hemoglobin released relative to total content. These methods provide a direct measure of sublethal damage accumulation, with hemolysis indices below 2% typically indicating robust mechanical stability in healthy cells. Quantitative evaluation often relies on ektacytometry, a laser diffraction-based technique that assesses cell elongation under varying shear stresses in a high-viscosity medium. The elongation index (EI) is computed as \text{EI} = \frac{L - W}{L + W}, where L and W represent the length and width of the diffracted laser pattern from deformed erythrocytes. Real-time monitoring via laser diffraction captures dynamic shape changes, enabling deformability curves across shear stresses from 0.3 to 300 Pa. For healthy erythrocytes, normal thresholds include an EI maximum exceeding 0.5 at physiological shear rates equivalent to 100–500 s⁻¹, with values below this indicating increased fragility. This approach overlaps conceptually with broader deformability metrics but specifically isolates mechanical stress responses. Despite their utility, these techniques exhibit limitations, including variability due to ex vivo conditions such as temperature fluctuations and sample handling, which can alter membrane integrity by up to 10–15%. Emerging methods from the 2020s, like atomic force microscopy (AFM), address this by applying picoNewton-scale forces to individual cells, probing local membrane stiffness and rupture thresholds with nanometer resolution, though scalability remains a challenge for population-level analysis.

Clinical applications

Assessment of erythrocyte mechanical fragility plays a crucial role in evaluating conditions characterized by circulatory trauma, where high shear stresses lead to red blood cell (RBC) fragmentation and hemolysis. In patients with prosthetic heart valves, elevated mechanical fragility contributes to schistocyte formation, resulting in intravascular hemolysis and hemolytic anemia. This mechanical damage arises from turbulent flow and high shear rates around the valve apparatus, often necessitating monitoring of plasma free hemoglobin levels to assess severity. Similarly, in sickle cell disease, sickled RBCs exhibit increased mechanical fragility under high shear conditions during vaso-occlusive crises, exacerbating hemolysis and contributing to chronic anemia and painful episodes. Mechanical fragility testing is employed in clinical monitoring to predict and manage hemolysis risks in vulnerable populations. Pre-surgical evaluation using RBC mechanical fragility metrics helps assess patient suitability for mechanical heart support devices, such as left ventricular assist devices (LVADs), by identifying those at higher risk of post-implantation hemolysis. Post-transfusion, elevated mechanical fragility in stored or patient RBCs correlates with increased hemolysis risk, guiding transfusion strategies to minimize extravascular destruction in fragile populations. Recent 2020s studies have linked COVID-19-associated coagulopathy to heightened RBC shear vulnerability, with altered deformability and aggregation under stress contributing to thrombotic complications and impaired oxygen delivery. Interventions targeting mechanical fragility focus on mitigating shear-induced damage. The design of low-shear blood pumps, such as centrifugal LVADs with optimized impeller geometries, reduces hemolysis by minimizing peak shear stresses and exposure times, improving long-term device hemocompatibility. Antiplatelet therapy, often combined with anticoagulation in prosthetic valve patients or sickle cell disease, helps reduce secondary mechanical damage by inhibiting platelet aggregation that amplifies shear-related RBC injury and thrombosis.

Influencing factors

Physiological influences

Erythrocyte fragility varies with the age and maturation stage of red blood cells. Reticulocytes, as immature forms, typically display lower osmotic fragility than fully mature erythrocytes due to their larger surface-to-volume ratio and active membrane remodeling processes that maintain structural integrity during early circulation. As erythrocytes age within the bloodstream, progressive membrane loss reduces surface area relative to volume, resulting in increased osmotic fragility and heightened susceptibility to lysis.^[29] Neonatal erythrocytes exhibit greater resistance to osmotic stress compared to those in adults, primarily owing to elevated levels of fetal hemoglobin (HbF). HbF influences intracellular hydration and membrane-cytoskeleton interactions, conferring enhanced stability against hypotonic conditions during the early postnatal period. This resistance diminishes as HbF is replaced by adult hemoglobin over the first few months of life.^[30]^[31] Hormonal factors, particularly cortisol, exert effects on erythrocyte membrane stability through direct interactions with lipid and protein components. Cortisol binds to the membrane with high affinity, inducing structural changes such as domain formation and alterations in surface topography, which can modulate overall membrane rigidity and fragility under physiological stress.^[32] Metabolic conditions, including glucose availability, significantly influence erythrocyte fragility by supporting energy-dependent maintenance of cell volume. Glucose fuels glycolysis to produce ATP, which powers ion pumps like Na+/K+-ATPase; reduced glucose levels compromise these pumps, leading to ion imbalances, cellular swelling, and elevated osmotic fragility.^[4] Environmental adaptations, such as exposure to high altitude, can increase osmotic fragility due to hypoxia-induced polycythemia and erythrocyte morphological changes. Hypoxia at altitude stimulates increased synthesis of 2,3-bisphosphoglycerate (2,3-BPG), which binds deoxyhemoglobin to reduce oxygen affinity and enhance tissue delivery.^[33] Gender-related differences in erythrocyte fragility have been noted, often linked to hormonal variations. Some investigations indicate marginally higher osmotic fragility in females, potentially influenced by sex hormones that affect membrane composition, though results vary across studies and species.^[34]^[35]

Pathological alterations

Pathological alterations in erythrocyte fragility arise from various diseases and exposures that compromise the structural integrity of the red blood cell membrane and cytoskeleton, predisposing cells to premature hemolysis. In genetic disorders such as hereditary spherocytosis, mutations in genes encoding ankyrin-1 (ANK1) or spectrin (e.g., alpha-spectrin or beta-spectrin) disrupt the vertical linkages between the lipid bilayer and cytoskeleton, resulting in spherocyte formation and markedly increased osmotic fragility due to reduced surface area-to-volume ratio and impaired ability to withstand hypoosmotic stress.^[36] These defects lead to splenic sequestration and extravascular hemolysis, with osmotic fragility tests showing hemolysis thresholds shifted toward isotonic conditions compared to normal erythrocytes.^[37] Glucose-6-phosphate dehydrogenase (G6PD) deficiency, another inherited condition, heightens erythrocyte vulnerability to oxidative stress, enhancing mechanical fragility through impaired NADPH production and subsequent glutathione depletion, which fails to neutralize reactive oxygen species.^[38] Under mechanical shear or oxidative challenges, G6PD-deficient cells exhibit accelerated membrane lipid peroxidation and cytoskeletal cross-linking, increasing hemolysis rates; for instance, in vitro oxidative stress induces significantly higher hemolysis in G6PD A- erythrocytes with residual enzyme activity around 5%.^[39] This oxidative mechanical vulnerability contributes to acute hemolytic episodes triggered by infections or drugs, with stored G6PD-deficient erythrocytes showing progressive increases in both osmotic and mechanical fragility akin to storage lesions.^[40] Acquired conditions further exacerbate fragility by targeting membrane permeability or cytoskeletal dynamics. In malaria infection, Plasmodium falciparum induces new permeability pathways (NPPs) in the host erythrocyte membrane via the plasmodial surface anion channel, elevating permeability to anions, cations, and organic solutes, which renders infected cells osmotically fragile and prone to colloid osmotic lysis.^[41] This altered permeability facilitates nutrient uptake for the parasite but increases membrane tension and fragility, with infected erythrocytes displaying heightened osmotic fragility and surface loss leading to splenic clearance and hemolytic anemia.^[42] Similarly, lead poisoning stiffens the erythrocyte cytoskeleton through chronic exposure, elevating membrane rigidity as evidenced by increased fluorescence polarization of embedded probes (e.g., DPH anisotropy rising from 0.204 to 0.343), which correlates with shape alterations like echinocytosis and enhanced osmotic fragility (1.6-fold higher hemolysis).^[43] These changes impair deformability, promoting mechanical entrapment in microvasculature and contributing to lead-induced hemolytic anemia. Toxicological agents also induce fragility via oxidative and peroxidative mechanisms. Chronic alcohol consumption triggers erythrocyte membrane fragility through ethanol-induced lipid peroxidation, which depolarizes the lipid bilayer, alters fatty acid composition, and increases osmotic hemolysis susceptibility by compromising membrane fluidity and integrity.^[44] This oxidative damage elevates malondialdehyde levels as a peroxidation marker and promotes eryptosis-like changes, leading to hemolytic states in alcoholics; supplementation with antioxidants like vitamins C and E can mitigate these effects by restoring balance and reducing fragility.^[45] In oncology, chemotherapy agents such as paclitaxel, carboplatin, and doxorubicin directly impair erythrocyte biophysical properties, increasing osmotic fragility (e.g., H50 threshold decreased by 6.4 mOsmol with paclitaxel) through membrane alterations, swelling, and microparticle formation, while also elevating mechanical vulnerability as seen in microfluidics assays with 4.7–9.8% slow-moving cells and occlusions.^[46] Recent in vitro studies from 2023 highlight additive effects in drug combinations, linking these changes to chemotherapy-induced anemia via enhanced hemolysis and reduced deformability, though clinical thresholds vary by agent and dosage.^[46]

Membrane deformability

Membrane deformability is a critical property of erythrocytes that enables these cells to undergo reversible shape changes, facilitating their passage through narrow capillaries with diameters as small as 3-5 μm. This deformability is particularly evident in the tank-tread motion observed under shear flow, where the lipid bilayer of the membrane rotates continuously around the cytoskeleton without the entire cell tumbling, maintaining orientation and minimizing energy dissipation.^[47] This motion is essential for efficient microvascular perfusion and oxygen delivery, as rigid cells would impede blood flow.^[48] The mechanical basis of erythrocyte membrane deformability lies in its viscoelastic properties, primarily governed by the membrane viscosity and the bending modulus κ, which quantifies the energy required to curve the membrane and is approximately $10^{-19} J for healthy cells.^[49] The bending modulus arises from the composite structure of the lipid bilayer and underlying spectrin-actin cytoskeleton, providing resistance to deformation while allowing flexibility. Variations in spectrin density, a key cytoskeletal component, directly influence this deformability; higher spectrin densities can enhance membrane stiffness, reducing the cell's ability to elongate under stress, as demonstrated in models incorporating proteomic data on molecular length distributions.^[50] Membrane viscosity, influenced by lipid composition and cytoskeletal interactions, further modulates the rate of shape recovery post-deformation.^[51] Osmotic gradient ektacytometry serves as a primary method to quantify erythrocyte deformability, measuring the elongation index (EI) of cells subjected to constant shear stress across a range of suspending medium osmolalities.^[52] In this technique, laser diffraction patterns from deformed cells yield an osmolar deformability profile, revealing parameters such as maximum EI (indicative of optimal deformability) and osmolality at half-maximal EI (reflecting cellular hydration status). This approach distinguishes subtle impairments in deformability due to cytoskeletal alterations, such as reduced spectrin network density, from those caused by volume changes.^[53] While related to overall erythrocyte fragility, membrane deformability represents a distinct, non-destructive aspect of cellular mechanics; in aging red blood cells, progressive reductions in deformability—driven by cytoskeletal remodeling and increased density—occur prior to elevations in fragility, marking early stages of cellular senescence before reaching lysis thresholds.^[54] This temporal distinction underscores deformability's role as a sensitive indicator of membrane integrity in physiological and pathological contexts.

Cellular aggregation and adhesion

Erythrocyte aggregation primarily occurs through the formation of rouleaux, which are linear stacks of red blood cells (RBCs) mediated by plasma proteins such as fibrinogen. Fibrinogen acts as a bridging molecule, binding to sialic acid residues on the surfaces of adjacent RBCs via its central domain, thereby promoting reversible cell-cell adhesion under low shear conditions.^[55] This bridging mechanism is enhanced by the asymmetric charge distribution on the RBC membrane, allowing fibrinogen to form cross-links that stabilize aggregates, with critical detachment forces measured between 10-20 pN in healthy plasma.^[55] In contrast, RBC adhesion to the endothelium involves specific receptor-ligand interactions, particularly prominent in pathological states like sickle cell disease, where sickle RBCs bind to laminin in the subendothelial matrix via Lutheran/basal cell adhesion molecule (Lu/BCAM) and to endothelial cells through CD36-thrombospondin interactions.^[56] CD36 expression on sickle RBCs facilitates this adhesion, contributing to vaso-occlusion by anchoring cells to the vessel wall under physiological flow.^[56] Assessment of erythrocyte aggregation and adhesion relies on specialized techniques that quantify intercellular interactions under controlled conditions. Laser aggregometry, such as the Laser-assisted Optical Rotational Cell Analyzer (LORCA), measures aggregation kinetics by monitoring laser backscatter versus time, yielding parameters like aggregation half-time and index to evaluate the extent and rate of rouleaux formation.^[57] For adhesion, flow chamber assays simulate vascular shear stress by perfusing RBC suspensions over endothelial monolayers, with adherent cells counted after stepwise increases in wall shear stress (e.g., 0.02–0.12 Pa), revealing shear-dependent binding dynamics.^[58] These processes have significant implications for erythrocyte stability, as aggregation in low-flow states increases blood viscosity and promotes stasis, amplifying mechanical stress on RBCs and potentially exacerbating fragility through prolonged exposure to uneven shear forces.^[59] Unlike membrane deformability, which pertains to individual cell flexibility, aggregation and adhesion involve multicellular forces that can lead to collective instability, such as in hypoxic or inflammatory conditions where fibrinogen levels rise.^[59]

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The present study showed that ethanol-induced oxidative stress in erythrocytes can lead to haemolysis and membrane-specific injuries in erythrocytes of the ...
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Anticancer Drugs Paclitaxel, Carboplatin, Doxorubicin, and ... - NIH
Here, we investigated how frequently used chemotherapy drugs directly affect RBCs. Our results show that chemotherapeutic drugs, whose main task is to damage ...Missing: trials | Show results with:trials
[45]
Tank Treading of Optically Trapped Red Blood Cells in Shear Flow
Tank-treading (TT) motion is established in optically trapped, live red blood cells (RBCs) held in shear flow and is systematically investigated.
[46]
Full dynamics of a red blood cell in shear flow - PNAS
We show that contrary to common belief, when red blood cells flip into the flow, their orientation is determined by the shear rate.<|control11|><|separator|>
[47]
Atomic force pulling: probing the local elasticity of the cell membrane
The local use of this methodology for determining the bending modulus of the cell membrane of the human erythrocyte yields a value of (2.07+/-0.32) x 10(-19) J.
[48]
Constitutive Model of Erythrocyte Membranes with Distributions of ...
We show that for the higher spectrin densities indicated by proteomics, accounting for a distribution of molecular lengths in the resting state is essential ...
[49]
ERYTHROCYTE MEMBRANE ELASTICITY AND VISCOSITY
For a shear elastic modulus of 6 X 10-3. mN/m, the bending modulus has to be about-1O-19 N m (10-12 ergs) for the cell to swell smoothly (without popping) from ...
[50]
Osmotic gradient ektacytometry: A valuable screening test ... - PubMed
Introduction: New generation osmotic gradient ektacytometry has become a powerful procedure for measuring red blood cell deformability and therefore for the ...
[51]
comprehensive characterization of red cell volume and surface ...
May 1, 1983 · Whole cell deformability of red cells was measured as a continuous function of suspending medium osmolality using the ektacytometer, ...
[52]
The Effect of the Aging of Red Blood Cells on the Ability of ...
Aug 6, 2025 · The objective of this study is to clarify the effect of the aging of RBCs on the ability of aggregation, fragility and deformability. Initially, ...
[53]
Quantifying Fibrinogen-Dependent Aggregation of Red Blood Cells ...
The fibrinogen molecule is considered to be the major plasma protein promoting RBC rouleau formation (22), and the synthetic polymer dextran can also promote ...
[54]
Intercellular adhesion molecule-4 and CD36 are implicated in ... - PMC
Abnormal adhesiveness of red blood cells to endothelium has been implicated in vaso-occlusive crisis of sickle cell disease. The present study examined ...
[55]
The Laser-assisted Optical Rotational Cell Analyzer (LORCA) as red ...
The Laser-assisted Optical Rotational Cell Analyzer (LORCA) is unique in its capacity to measure at least two important hemorheological parameters.
[56]
Specific Binding of Red Blood Cells to Endothelial Cells Is ... - NIH
Flow Chamber Adhesion Assay. The flow system consisted of an acrylic flow deck and a silicone rubber gasket (Glycotech) with the cut out area of the gasket ...
[57]
The Impact of Biophysical Properties of Erythrocytes on their ... - NIH
Erythrocyte aggregation is one of the major determinants of in vivo blood flow and blood viscosity at low shear rates. During the aggregation process ...Missing: implications | Show results with:implications

Erythrocyte fragility

Overview

Definition and physiological role

Historical development

Osmotic fragility

Underlying mechanisms

Measurement techniques

Clinical applications

Mechanical fragility

Underlying mechanisms

Measurement techniques

Clinical applications

Influencing factors

Physiological influences

Pathological alterations

Related erythrocyte properties

Membrane deformability

Cellular aggregation and adhesion

References