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5 April 2026

From Phytotoxin to Cell-Death Probe: Ophiobolin A and Related Sesterterpenoids in Membrane Stress and Non-Apoptotic Cell Death

,
and
1
Department of Photomedicine and Physical Chemistry, Medical College, University of Rzeszów, 35-025 Rzeszów, Poland
2
English Division Science Club, Medical College, University of Rzeszów, 35-025 Rzeszów, Poland
3
Department of Biochemistry and General Chemistry, Medical College, University of Rzeszów, 35-025 Rzeszów, Poland
*
Authors to whom correspondence should be addressed.

Abstract

Ophiobolin A is a fungal sesterterpenoid initially characterised as a phytotoxin but progressively investigated for its biomedical significance due to its potent and mechanistically characteristic cellular activities. In this review, Ophiobolin A is discussed within the wider landscape of natural products as a source of bioactive molecular scaffolds, and current knowledge on its structural features, biosynthesis, chemical synthesis, semi-synthetic modification, and in vitro biological applications is summarised. Evidence drawn from chemical, biochemical, and cell biology studies is integrated to describe the distinctive 5-8-5 tricyclic scaffold, the electrophilic dicarbonyl motif, and their roles in covalent modification of cellular components. Collectively, the reviewed evidence underscores that Ophiobolin A and its derivatives trigger both apoptotic and non-apoptotic cell death pathways. These include paraptosis-like death, which is a regulated form of cell death not associated with apoptosis that is defined by major cytoplasmic vacoulisation. This commonly occurs in apoptosis-resistant cancer models via disruption of membrane lipid homeostasis, calmodulin-dependent signalling, mitochondrial function, and proteostasis. Structure–activity relationship studies show that modulation of electrophilicity, oxidation state, and peripheral functionality enables tuning of potency, selectivity, and traceability while retaining key phenotypes. In addition to anticancer effects, antimicrobial and anti-inflammatory activities are also briefly summarised. Taken together, the literature supports Ophiobolin A as a useful molecular probe for considering cell death mechanisms and as a chemically complex yet suitable starting point for derivative development, while reinforcing the need for improved selectivity, delivery strategies, and in vivo validation to further translational potential.

1. Introduction

Both as approved drugs and as chemical frameworks that provide a structural basis for semi-synthetic or fully synthetic analogues, an extremely large share of clinically useful chemical matter continues to be provided by natural products. The ability of evolutionarily selected metabolites to involve complex biology with high ligand efficiency and structural uniqueness is reflected by large-scale analyses of modern approvals highlighting “natural product” origin as a dominant theme in oncology and anti-infectives [1]. Simultaneously, the discovery process has been strengthened by methodological advances in genome mining, metabolomics, and high-content phenotypic screening, which has enabled faster linkage of bioactivity to structure and biosynthetic origin [2]. Fungal secondary metabolites occupy an advantaged position in this field, as chemically dense and stereochemically rich frameworks are regularly produced by fungi. They often contain electrophilic functionalities and unique ring systems, which are highly effective at disrupting eukaryotic signalling and membrane homeostasis.
Within the class of fungal terpenoids, ophiobolins represent a family of C25 characteristic sesterterpenoids. They were initially recognised for their phytotoxicity but are increasingly investigated for their biomedical potential. Marine-derived fungi are a widely recognised source of chemically reactive anticancer frameworks, especially terpenoids that elicit non-apoptotic stress responses. Ophiobolins are consistent with this broader marine-fungal pattern of cytotoxicity, which is led by membrane and organelle disruption instead of single-protein inhibition [3]. The first structural characterisation of the class can be traced to classic isolation and structure elucidation work by Nozoe et al., who established a new framework in terpene chemistry when they reported the novel carbon skeleton of ophiobolin in the mid-1960s [4]. The family of plant-pathogenic and endophytic fungi, such as Bipolaris and Drechslera, has been expanded in subsequent studies. Additionally, the wide range of activities in plants, microbes, and mammalian systems has been emphasised in comprehensive biological summaries. This positions Ophiobolin A (OpA) as a key reference for mechanism-of-action studies [5]. Many natural congeners are now catalogued in modern overviews, which highlight how bioactivity profiles can be significantly reshaped by stereochemical and oxidation-state differences [6,7]. Even within the ophiobolin family, OpA is chemically unique. OpA is characterised by a distinctive tricyclic 5-8-5 fused ring system. It consists of a cyclooctane embedded within a compact polycyclic structure, coupled with a dense array of oxygenated functionality and reactive carbonyl motifs. These features collectively establish OpA as a conformationally constrained, three-dimensional molecular scaffold [6]. Both the structural conversion of the 5-8-5 core and the variation in peripheral oxidation patterns across producing strains can be rationalised by biosynthetic analyses. This provides clarification for this architecture arising from specialised sesterterpene cyclisation pathways, frequently involving bifunctional enzymes that pair prenyl chain assembly and cyclisation [8].
OpA’s integration of a rigid polycyclic backbone and selectively positioned electrophiles is especially noteworthy from a medicinal chemistry perspective. OpA can support both high-affinity noncovalent recognition and covalent modification of nucleophilic protein residues. These are attributes that can translate into pronounced, pathway-selective phenotypes but also require cautious profiling for off-target reactivity. Previously, OpA’s inhibition of calmodulin-dependent processes was seen to drive mechanistic interest. It was demonstrated in early biochemical studies that calmodulin-activated cyclic nucleotide phosphodiesterase is strongly inhibited by OpA [9], whereas in follow-up work, calmodulin inhibition was linked to phytotoxicity, and specific lysine residues involved in binding and inactivation were mapped [10,11]. In modern target-discovery efforts, this ability for covalent or quasi-covalent engagement has been persistently observed, including in recent chemoproteomic studies that facilitate a broader interrogation of proteome-wide reactivity and downstream effects on cancer cell viability [12]. Cell biology studies have simultaneously demonstrated that in apoptosis-resistant contexts, OpA can stimulate non-apoptotic cell death programmes. For example, paraptosis-like death, a non-apoptotic cell death phenotype associated with vacuolisation, has been observed in glioblastoma models. This positions OpA as a promising lead for the treatment of challenging malignancies [13]. These developments are synthesised in current reviews, and the evolving therapeutic framework is highlighted, which is that, through mechanism-guided optimisation and derivative design, a fungal phytotoxin scaffold is being recontextualised. It is now being considered for therapeutic application as a starting point for anticancer and other potential medical applications [14].

2. Materials and Methods

PRISMA guidelines for literature identification and selection were followed in this review. Studies on Ophiobolin A and related congeners using structure-, mechanism-, and application-focused keywords were searched for on PubMed and PubMed Central (PMC). Articles were screened by title and abstract, followed by evaluation of the full text for relevance to biosynthesis, chemical modification and biological activity in vitro. The PRISMA flow diagram in Figure 1 summarises the study selection process.
Figure 1. PRISMA flow diagram of literature selection. Flowchart showing the identification, screening, eligibility assessment, and inclusion of studies retrieved from PubMed and PMC for this review. The mark (*) means the total number of recognized records. The mark (**) means the total number of excluded records.

3. Biosynthetic Origin, Structural Features, and Ecological Roles of Ophiobolins

Ophiobolins are sesterterpenoids most frequently derived from plant-associated filamentous fungi. Mangrove-derived endophytic fungi represent an important source, frequently producing several new ophiobolin congeners from a single strain, emphasising their value for scaffold diversification [15]. Ophiobolins act as phytotoxins that cause necrotic lesions and contribute to disease symptoms in cereals and grasses in classic producer genera, including Bipolaris spp. and Drechslera spp., such as B. maydis, B. sorokiniana, and B. setariae [16]. 3-anhydro-ophiobolin A and 6-epi-ophiobolin A were put forward as significant determinants of pathogenicity in Bipolaris setariae, supporting a direct ecological role in host colonisation [17]. Genetics have identified many biosynthetic gene clusters and a bifunctional ophiobolin synthase that assists ophiobolin biosynthesis and diversification within Aspergillus spp. This establishes Aspergillus spp. as another important source, which includes mangrove-sourced Aspergillus ustus and endophytic Aspergillus calidoustus [18]. Ophiobolin K from A. ustus displays antibacterial and antifungal activity, suggestive of an ecological defence function. This demonstrates that ecologically, beyond plant pathogenesis, ophiobolins can function as chemical defence agents in microbial competition [19]. These ecological roles explain why ophiobolins are highly active, membrane-reactive cytotoxins in vitro, and why viable synthetic pathways to the supply of OpA and its related congeners for pharmacology include fermentation, strain engineering, and semi-synthesis from fungal extracts [20].
OpA is a C25 sesterterpenoid underpinned by a distinctive 5-8-5 tricyclic carbon skeleton (A-B-C ring system) that rigidly displays substituents and supports semi-synthetic modification for therapeutic lead discovery [21]. OpA’s electrophilic unsaturated 1,4-ketoaldehyde/1,4-dicarbonyl region, which consists of an enal adjacent to a ketone, is the main bioactivity hotspot. Pyrrole-type covalent adducts are formed when this motif reacts with primary amines, and covalent modification of phosphatidylethanolamine (PE) links it to cytotoxicity [22]. It is demonstrated in recent semi-synthetic structure–activity relationship (SAR) studies that both potency and selectivity correlate with preservation of the electrophilic unsaturated dicarbonyl motif [23]. Relative to other ophiobolins, oxidation patterns, double-bond placement, and stereochemistry, which regulate electrophilicity and 3D shape, differ between congeners, although they share the same 5-8-5 core. These variations are related to distinct anti-proliferative, phytotoxic, and antimicrobial profiles in reviews contrasting OpA with ophiobolins B/C and other members [6]. Stereodefined access for probe design is provided by total syntheses, and bicyclic derivatives that retain anticancer activity, providing a foundation for scaffold-based medicinal chemistry, are yielded by pharmacophore-guided simplification [24]. OpA efficiency against drug-resistant cells in glioblastoma models has prompted derivative programmes. Recent OpA derivatives with improved activity under tumour-microenvironment conditions show that adjusting peripheral oxidation while retaining the reactive dicarbonyl can improve performance without disrupting the ophiobolin topology [25]. This enables synthetic–biological iteration for in vitro translation.
OpA is biosynthesised from geranylfarnesyl diphosphate (GFPP) and belongs to the fungal sesterterpenes (C25). Terpene cyclisation catalysed by a bifunctional sesterterpene synthase, commonly referred to as ophiobolin synthase, constructs the characteristic 5-8-5 tricyclic. GFPP is assembled by a prenyltransferase domain. A cationic cyclisation and rearrangement cascade that forms the 5-8-5 core is triggered by a terpene cyclase domain [8], as shown in Figure 2. In Aspergillus and Bipolaris, biosynthetic gene clusters (BGCs) that encode this machinery have been characterised. In several Bipolaris spp., comparative genomics has localised conserved ophiobolin BGC regions, supporting an evolutionarily conserved biosynthetic strategy to produce these bioactive metabolites [26]. Studies demonstrate that in Aspergillus ustus production of ophiobolin relies on the C25 synthase gene, together with coordinated activity from additional terpene-related clusters. This emphasises pathway-level regulation instead of single-enzyme limitation [18]. Current genome-guided surveys of Aspergillus secondary metabolism suggest that terpenoid biosynthetic diversity continues to grow, strengthening the usefulness of cluster-driven exploration for new ophiobolin congeners [27]. Subsequently, oxidation patterns that correlate with OpA and derivative bioactivity in vitro could be introduced by tailoring enzymes, particularly cytochrome p450 monooxygenases and flavin-dependent oxidases [28]. Light conditions can regulate OpA production in Bipolaris maydis, which is relevant to fermentation optimisation for supplying material for semi-synthesis and pharmacology, demonstrating regulation is environmentally responsive [29]. These structure–biosynthesis–regulation relationships are summarised in Table 1. Furthermore, scalable access for medical and mechanistic studies is supported by synthetic biology efforts that establish de novo biosynthesis of ophiobolin-type sesterterpenoids [21].
Figure 2. Structural architecture and biosynthetic origin of Ophiobolin A. (A) Core chemical structure highlighting the 5–8–5 tricyclic scaffold and electrophilic motif; (B) Biosynthetic formation of the tricyclic core from geranylfarnesyl diphosphate (GFPP); (C) Tailoring reactions generating ophiobolin congeners; (D) Cellular reactivity leading to membrane disruption, ER stress, and paraptosis-like cell death. Created in BioRender. Wilk, I. (2026) https://BioRender.com/49l1lck.
Table 1. Key structural elements of Ophiobolin A: biosynthetic origin, chemical reactivity, and functional consequences. Abbreviations: flavin adenine dinucleotide (FAD), mechanism of action (MoA).

4. Chemical Synthesis and Semi-Synthetic Derivatives of Ophiobolin A

4.1. Total Synthesis Strategies and Stereochemical Challenges

The total synthesis of OpA is challenging due to the regulation of dense stereochemistry. In many structural analogues, a spirocyclic ether (5-8-5-5) is incorporated into the framework, while the 5-8-5 fused carbocyclic core is assembled. Due to unfavourable entropic contributions, transannular interactions, and alternative rearrangement pathways during medium-ring formation, the highly substituted eight-membered ring is a constant synthetic limitation [30]. Early ophiobolin nucleus construction studies that established feasible strategies for building the tricyclic framework are considered key milestones [32]. A major recent advance was the convergent and enantiocontrolled total synthesis of (+)-OpA by Tsuna et al. It combined stereoselective Hosomi–Sakurai cyclisation to establish the spiro-fused C-D ring system, fragment coupling to install the A ring, and olefin-metathesis-mediated ring formation. This demonstrated a framework for constructing the full ophiobolin structure [24,30]. In recent years a simplified platform that resolved the spirocyclic tetrahydrofuran and stereochemical problems with reduced step count was provided by a 14-step total synthesis of (+)-6-epi-ophioblin A [31]. With respect to yield and scalability, total synthesis continues to be multi-step with modest overall yield. Therefore, fermentation or isolation followed by semi-synthesis is frequently preferred for providing OpA and its analogues for in vitro pharmacology. Nevertheless, synthetic throughput can be improved by more recent cascade or cyclisation strategies that quickly access 5-8-5 tricycles, facilitating medicinal chemistry diversification under conditions of inadequate natural supply [33].

4.2. Semi-Synthetic Modification Axes for Biological and Medicinal Studies

Semi-synthetic approaches are essential to translating OpA into practical in vitro tools and medicinal leads. The natural product is generally poorly water-soluble as well as highly electrophilic. However, its activity can be strongly impacted by small structural changes. OpA’s covalent reactivity, exemplified by the pyrrolylation of PE, and its cytotoxicity are predominantly determined by a first modification axis, which targets functional groups around the defining unsaturated aldehyde/ketone, 1,4-dicarbonyl, region [7]. The ketone and enal/aldehyde moieties have been systematically modified in recent semi-synthetic SAR studies. This involved selective reduction, oxidation, and derivatisation, showing that reducing electrophilicity can improve handling. However, this often decreases biological activity, which is valuable for separating reactivity from activity when designing probes [23]. Solubility and chemical stability aim to be improved by a second axis, without fully eliminating the pharmacophore. Common strategies include introducing ester/ether handles, installing polar linkers, or formulating prodrug-like derivatives, such as amino-acid or ionisable motifs, to increase aqueous solubility and decrease nonspecific compound loss during administration. These strategies are commonly used for poorly soluble electrophiles and can be optimised for derivatisation campaigns [34]. Adjusting of polarity and reactivity while preserving anti-proliferative activity against apoptosis-resistant cancer cells can be enabled by converting the reactive motif into unsaturated ester derivatives and even dimeric constructs in OpA-specific work [35]. Lastly, analogue-library generation directly from isolated OpA is supported by semi-synthesis. Derivatives with enhanced activity under tumour-microenvironment conditions have been produced from focused libraries that vary oxidation state, electrophile presentation, and linker design, generating traceable sets for mechanism-of-action and lead optimisation studies in vitro [25].

4.3. Structure–Activity Relationships Governing Electrophilicity and Cytotoxicity

Cytotoxicity is constantly traced to preservation of an electrophilic C5, C21 “dicarbonyl” region that functionally links the A-ring enone/ketone chemistry with the C21 aldehyde in SAR studies of OpA. When comparing natural congeners and early semi-synthetic analogues, studies indicate that alterations in stereochemistry or conjugation around this motif, e.g., 6-epi- and anhydro-OpA, significantly decrease activity. However, removing one carbonyl, such as by the reduction of the C21 aldehyde, can abolish activity completely. This suggests that this electrophile set is an essential requirement for marked anticancer effects. At the mechanistic level the aldehyde is not just a functionalisation site, but together with the adjacent carbonyls it also allows covalent chemistry in cells. With primary amines, OpA can undergo Paal–Knorr-type pyrrolyation, and cytotoxic covalent adducts can be formed with PE, which is a link correlated with paraptosis-like death in apoptosis-resistant cancer models [36]. Covalent modification of nucleophilic residues, such as lysines via Schiff-base-type chemistry, is also described in target-directed studies [12]. Modern derivatisation that selectively varies oxidation state at the ketone and the unsaturated aldehyde further supports the conclusion that adjusting electrophilicity tunes cytotoxicity toward breast cancer and glioblastoma stem-like cells [23]. Thus, pharmacophore proposals highlight the 1,4-keto or unsaturated aldehyde electrophile set with greater tolerance for modifications at the distal side chain in addition to the correct C5/C6 stereochemistry and topology of the A/B ring system and supportive C3 oxygenation. More generally, sesterterpenoids are increasingly acknowledged as a pharmacologically relevant class in oncology, supporting SAR efforts aimed at maintaining anticancer activity whilst reducing nonspecific reactivity [37]. OpA-focused SAR analyses do not identify an epoxide as a critical feature. Epoxides are best regarded as conformation or reactivity modulators when introduced in derivatives, rather than primary cytotoxic drivers [38]. The key electrophile-based modification strategies, design rationales, and associated biological consequences described above are summarised in Table 2 and Figure 3.
Table 2. Synthetic and semi-synthetic functionalisation map for OpA, describing what has been altered, how, and which biological or chemical readouts support these design choices. Abbreviations: calmodulin (CaM), C/EBP homologous protein (CHOP), glioblastoma (GBM).
Figure 3. Synthetic access and semi-synthetic derivatisation landscape of Ophiobolin A. The preserved 5–8–5 Ophiobolin A scaffold acts as a hub for total synthesis and semi-synthetic strategies that adjust electrophilicity, redox state, and polarity, leading to biological phenotype shifts and optimisation of potency, selectivity, and usability. Created in BioRender. Wilk, I. (2026) https://BioRender.com/adtasa2.

5. Molecular Targets and Mechanism of Action of Ophiobolin A

5.1. Membrane and Cytoskeletal Disruption via Covalent Lipid and Protein Engagement

OpA and semi-synthetic derivatives are commonly positioned as covalent, mechanism-guided leads in clinically orientated in vitro studies. Strong anticancer phenotypes and toxicity risks can be explained by their electrophilic motifs, which can disrupt membranes and cytoskeletal signalling. Disturbance of early secretory pathway function is known to increase endoplasmic reticulum (ER) stress and proteostasis collapse, offering a complementary framework for understanding ophiobolin-induced cytotoxicity [42]. Lipid targeting is a key membrane mechanism. OpA generates a pyrrole-containing covalent adduct with PE in human cells. This directly modifies a predominant inner-leaflet phospholipid and most likely alters bilayer structure, curvature, and the function of adjacent membrane proteins [22]. With respect to the cytoskeleton, calmodulin (CaM) is directly inhibited by OpA. CaM lysines that covalently bind OpA, specifically Lys-75 and Lys-148, were identified by site-directed mutagenesis and showed the primary inhibitory site to be Lys-75. Calcium ion (Ca2+)-dependent, effectively irreversible CaM inactivation was further supported by kinetic work [11]. This is significant because CaM is a vital regulator of actin dynamics. CaM has two ways of controlling actin organisation. The first is through the regulation of phosphatidylinositol-4,5-bisphosphate synthesis. The second is through the signalling of Ca2+/CaM-dependent myosin light chain kinase that modulates contractility and adhesion dynamics [43,44]. In line with these mechanistic connections, rapid, significant remodelling of F-actin, with reduced proliferation and migration, was exhibited in glioblastoma models treated with OpA in addition to a paraptosis-like vacuolisation process [13]. Collectively, membrane microenvironments can be destabilised by PE adduction, whilst actin assembly and force generation can be disrupted by CaM blockade. The combined effects can decouple the plasma membrane from the actin cortex, disrupt intracellular trafficking, and reduce cell motility. A reasoned route to derivatives with improved selectivity for therapeutic applications in synthesis efforts is tuning electrophilicity or sterics to favour PE versus CaM reactivity. Given that certain tumours externalise PE, OpA-like molecular frameworks have been described as chemical probes or payloads. This is because OpA can make use of this membrane lipid profile, although off-target concerns are also raised by covalent lipid chemistry [45].

5.2. Engagement of Multiple Regulated Cell Death Pathways

OpA and semi-synthetic derivatives can push cancer cells into distinct cell death pathways. This is useful when a tumour has inactivated one pathway and makes them appealing in medicinally orientated in vitro work. OpA can activate intrinsic (mitochondrial) apoptosis in apoptosis-proficient cells, whereas OpA induces mitochondrial compromise with autophagy: integration of apoptotic signalling with downstream caspase activation in melanoma [46]. Many ophiobolins, such as A, B, C and K, trigger apoptotic death at nanomolar concentrations in leukaemia-focused screens, confirming that apoptosis is a readily targetable outcome for this scaffold class [47]. Ophiobolin O alternatively exemplifies how structurally related congeners can direct cell death. This occurs through mitogen-activated protein kinase (MAPK)-linked apoptosis and by the inhibition of the cell cycle in breast cancer cells, including in chemo-resistant contexts [48,49,50]. As many solid tumours resist caspase-dependent death, non-apoptotic pathways are equally important, as shown in Figure 4. An apoptosis-bypass option is offered by paraptosis, which is defined as a programmed, caspase-independent vacuolating death with swelling and dilation of mitochondria and sometimes the endoplasmic reticulum. Paraptosis is progressively recognised as a therapeutically significant alternative to apoptosis, especially in apoptosis-resistant tumours, and is commonly stimulated by natural products that target organelle homeostasis [51]. MAPKs regulate paraptosis, and apoptosis-inducing protein-1 (AIP-1/Alix) inhibits it [52]. These phenotypes are connected by organellar stress biology. Continued unfolded-protein response signalling can shift from adaptation to pro-death outputs [53]. Meanwhile, reactive oxygen species (ROS)-driven lipid peroxidation and bioenergetic failure are amplified by mitochondrial redox imbalance [54]. In this context reactive oxygen species (ROS) accumulation and adenosine triphosphate (ATP) depletion would be expected to be intensified by diminishing of mitochondrial respiratory capacity with disruption of complex IV-dependent electron transport. This reinforces potentiating bioenergetic stress as opposed to acting as an isolated cytotoxic trigger [12]. The observed integration of redox imbalance, organellar dysfunction, and controlled cell death outcomes described for OpA-treated cells aligns with such a mitochondrial respiratory interference. A complementary, iron-dependent lipid-peroxidation death axis is added by ferroptosis, which is regulated by the cystine/glutamate antiporter (system xC)/reduced glutathione (GSH)/glutathione peroxidase 4 (GPX4) [55,56], and lipid peroxidation is a terminal biochemical event across multiple regulated cell death pathways [57]. The practical implication for ophiobolin medicinal chemistry is to profile caspases, vacuolisation or ER dilation, and ferroptosis markers across tumour states, e.g., epithelial–mesenchymal transition (EMT)-enriched breast cancer cells. This is because cell death pathway engagement varies with cellular context and can be altered by minor structural modifications [58]. Assessing OpA phenotypes benefits from the Nomenclature Committee on Cell Death (NCCD) system for classifying regulated cell death across studies, leading to caspase activation, plasma-membrane rupture, or lipid-ROS accumulation not being inferred from single markers [59]. Links between synthetic modifications and mechanisms are strengthened by multiparametric analyses such as these.
Figure 4. Multi-axis molecular stress propagation triggered by Ophiobolin A. Ophiobolin A induces parallel membrane, Ca2+, mitochondrial, and proteostasis stresses that converge on signalling collapse and integrated stress responses, leading to apoptosis, paraptosis, or lipid-peroxidation-associated cell death in a context-dependent manner. Created in BioRender. Wilk, I. (2026) https://BioRender.com/06wc560.

5.3. Modulation of Pro-Survival and Stress-Responsive Signalling Networks

OpA and medicinally altered derivatives regulate several important signalling axes instead of a single node in cancer-orientated in vitro studies. OpA was described to simultaneously inhibit phosphoinositide 3-kinase (PI3K)/mechanistic target of rapamycin (mTOR) and Ras/Raf/extracellular signal-regulated kinase (ERK) pathway output. This reduces the phosphorylation of protein kinase B (Akt), ribosomal protein S6 (S6) and ERK. Additionally, this diminishes cyclin-dependent kinases (CDKs) and retinoblastoma protein cell-cycle signalling, which are routinely used as phosphor markers in SAR work [60]. Alterations in Akt markers help position OpA analogues against pro-survival signalling pathways because PI3K-Akt generally supports proliferation and survival [61]. So that OpA-driven perturbations can activate both mitogenic and stress-activated pathways, mitogen-activated protein kinase (MAPK) modules, such as ERK, c-Jun N-terminal kinase (JNK), and p38, can combine growth cues with stress responses [62]. Sustained stress is often interpreted by tumour cells via the integrated stress response, which can steer adaptive signalling toward death when damage is excessive [63]. Marine-fungal metabolites often activate stress-response signalling rather than single linear pathways, supporting the interpretation of ophiobolins as multidimensional stress inducers [64]. A second regulatory mechanism is calcium homeostasis. OpA is a covalent CaM inhibitor; CaM-dependent signalling is associated with tumour migration and invasiveness [65]. CaM antagonism is also closely linked to cancer cell migration and stress adaptation, offering a mechanistic bridge between ophiobolin exposure and invasive phenotypes [66]. More precise analysis of Ca2+- and CaM-linked signalling effects is enabled by a less toxic OpA analogue developed as a CaM-directed chemical probe in K-Ras contexts [67]. Combining phospho-profiling with live Ca2+ flux assays strengthens mechanistic interpretation since altered Ca2+ signalling forms the basis of multiple key cancer features. Derivatives for combination therapy can therefore be selectively prioritised [68]. This can be done using combined phospho-signalling and Ca2+ flux profiling, in accordance with the integrated target and pathway structure summarised in Table 3.
Table 3. Molecular targets and mechanistic nodes engaged by OpA in mammalian cells: direct covalent interactions, pathway outputs, and phenotypic consequences. Abbreviations: large-conductance Ca2+-activated potassium channel (BKCa), cancer stem cell (CSC), liquid chromatography–tandem mass spectrometry (LC-MS/MS), oxygen consumption rate (OCR), retinoblastoma protein (RB), cytochrome c oxidase subunit 5A (COX5A), hypoxia-inducible gene domain family member 2A (HIGD2A), mitochondrial membrane potential (ΔΨm).

7. Preclinical Therapeutic Potential and Translational Challenges of Ophiobolin A

OpA and closely related ophiobolin structures are relevant in preclinical models because of their ability to kill tumour cells. They achieve this by mechanisms different from traditional DNA-damaging or microtubule-targeting anticancer drugs. OpA’s activity in chemo-resistant stem-like states is explained by being highlighted as a CSC target. OpA targets these cells through the disruption of K-Ras and calmodulin signalling, instead of targeting faster dividing cells first [86]. Ophiobolin chemistry enables more extensive covalent engagement of nucleophile-rich biomolecules, such as primary amines. This is a property that is increasingly used in probe and derivative design but also requires careful safety pharmacology [87]. Advantages of OpA over conventional cytotoxics include its potential efficacy in apoptosis-resistant contexts. Its potential for pathway-selective phenotypes, such as Ras- or CaM-linked stemness, instead of uniform mitotic arrest is also advantageous [88]. However, there are still preclinical limitations, such as selectivity and potency. Ophiobolins can have effects across a variety of eukaryotic cells. Therefore, therapeutic windows must be engineered by delivery, masking, or context-activated derivatives and benchmarked against normal-cell liabilities [89,90]. EMT-state-dependent redox responses reported for OpA imply that cell state may modify sensitivity. This is important for biomarker-led development [78,91].
Toxicity, therapeutic window, stability, and delivery constraints dominate the translation of OpA and derivatives from potent in vitro cytotoxins into drug candidates. There is a risk of widespread, mechanism-independent reactivity in normal tissues implied by OpA’s electrophilic motifs. Recent experiences with covalent drugs show that to avoid off-target protein or lipid alkylation and dose-limiting toxicity, warhead reactivity must be tuned. Tuning can occur using kinetics, selectivity and exposure [92,93]. Therefore, when prioritising OpA derivatives, measuring and evaluating electrophile reactivity, including fragment or warhead profiling concepts, is essential [94]. Aldehyde or Michael chemistry can produce adducts with nucleophilic residues. Due to this, systemic inflammation or liabilities remain likely and careful in vivo tolerability studies are required [95]. The importance of defining exposure-response relationships and safety margins was emphasised in a small animal study. The conclusion of the study was that OpA can trigger rapid inflammatory mediator release [96]. Lipophilicity and electrophilic instability, such as thiol- or amine-rich matrices, are followed by stability and delivery limitations. These limitations motivate formulation-led approaches to regulate biodistribution and decrease peak systemic exposure [97]. This is shown in Figure 6. Pharmacokinetic control, which includes slower release and lower Cmax, is conceptually attractive for reactive natural products. This can be provided by regional delivery platforms such as drug-eluting beads or microspheres [98,99,100].
Figure 6. From mechanistic potency to therapeutic translation: medical potential of Ophiobolin A. This figure compares strong mechanistic and in vitro anticancer activity, including efficacy in apoptosis-resistant and invasive cancer phenotypes, with a tight therapeutic window led by toxicity. Translational strategies such as nanocarrier encapsulation, prodrug masking, targeted delivery, and medicinal chemistry optimisation are emphasised as routes to advance clinical feasibility. Created in BioRender. Wilk, I. (2026) https://BioRender.com/dfcedeo.
OpA is shown to covalently target mitochondrial respiratory complex IV, causing a metabolic collapse in cancer cells. This feature of OpA slows down clinical translation. While in metabolically stressed tumours this mechanism may be of benefit, complex IV is essential in high-energy normal tissues. As a result, concerns are raised over on-target mitochondrial toxicity and narrowing the therapeutic window. Therefore, delivery strategies that are exposure-controlled are crucial to balance antitumour activity with systemic tolerability. Additionally, early mitochondrial safety profiling will also be a key factor [12].
Nanocarrier strategies for OpA are a relatively recent development. The aim of nanocarrier strategies is to solubilise OpA and derivatives, protect reactive motifs until the drug reaches the tumour, and to shape biodistribution. Liposomes are commonly used as delivery platforms, as they have well-known clinical validation. Liposomes can increase circulation time, reduce free-drug peaks, and enable surface engineering. The most common liposome surface modifications are polyethylene glycol (PEG) modification (PEGylation) or ligand presentation for tumour-specific uptake [101]. When using hydrophobic terpenoids like OpA, stability and tumour accumulation can be enhanced using lipid/polymer nanoparticles or hybrid systems. This can be further supported by the literature about terpenoid nano-formulation [102]. A way to combine enhanced permeability and retention (EPR)-based accumulation with deeper tumour penetration is offered by size- or charge-switching designs. pH-responsive shrinkable nanoparticles [103] are a good example of this type of delivery system. Together, prodrug and targeted delivery can mask OpA’s most reactive handles. This can be done with cleavable promoieties that unmask especially in tumours. For example, promoieties can be unmasked within reactive oxygen species (ROS)-rich reductive or enzyme-high microenvironments. This reduces the risk of off-target reactivity [104,105]. This approach complements emerging OpA biology in cancer cells. Moreover, the therapeutic index can be widened by pairing it with ligand targeting [106,107]. This is summarised in Table 5.
Table 5. Biological constraints and translational rationales governing therapeutic exploration of OpA and derivatives.

8. Discussion

8.1. Mechanistic Integration of Ophiobolin A Cytotoxicity

Together, the evidence reviewed here supports the conclusion that OpA and its congeners are fungal-derived small molecules with distinct anticancer activity, able to participate in mechanisms past standard apoptosis. OpA was shown to form cytotoxic adducts by covalently reacting with membrane PE in unbiased genetic screens, causing disruption of lipid bilayers and contributing to the selective killing of cancer cells, supporting earlier work in human haploid cells [22]. Alongside membrane reactivity, targeting of mitochondrial complex IV subunits has been reported in recent chemoproteomic studies. The COX5A and HIGD2A subunits of complex IV are frequently targeted. This leads to oxidative stress, compromised membrane potential, and ATP reduction [12]. The wider recognition that disrupting redox balance and membrane integrity can overthrow apoptotic resistance is supported by understandings of these core mechanisms, and they highlight the value of OpA as a molecular probe for alternative death pathways.

8.2. Ophiobolin A and Non-Apoptotic Cell Death Pathways

Many of the cellular responses caused by OpA align with established non-apoptotic cell death programmes. For instance, ferroptosis is characterised by iron-dependent lipid peroxidation and lethal membrane rupture; this is a mode of death separate from caspase-dependent apoptosis and progressively pursued for therapeutic gain in oncology [108,109]. Though direct evidence linking OpA cytotoxicity to canonical ferroptosis is yet to be established, the significance of membrane lipid interactions, mitochondrial dysfunction, and redox perturbation situates OpA within the conceptual framework of therapies that leverage ferroptotic vulnerabilities [108]. Canonical ferroptosis validation approaches should be applied to studies in the future to address this. These approaches include rescue experiments using ferroptosis inhibitors, like ferrostatin-1 or liproxstatin-1 [110], the assessment of iron dependency, and the quantification of lipid peroxidation using boron-dipyrromethene (BODIPY)-C11 oxidation. In addition, observing the activity of GPX4, glutathione decrease, and the function of system xC [111] would help to establish if OpA-induced cytotoxicity engages ferroptotic pathways.

8.3. Limitations and Knowledge Gaps

Significant limitations temper interpretation and translational promise, despite this convincing mechanistic landscape. Unfavourably, almost all available data is derived from in vitro models, restricting the confidence in the physiological relevance of the observed mechanisms, as depicted in Figure 7. Although one early study reported the antitumour effects of OpA in a mouse melanoma lung metastasis model, the data remains partial and has not been greatly replicated or supported through pharmacological characterisation [7]. Moreover, comprehensive pharmacokinetic (PK) and pharmacodynamic profiling of OpA and congeners is still absent, leaving many questions about bioavailability, metabolic stability, tissue distribution, and therapeutic index unanswered. Crucially, the OpA core seems to have a narrow therapeutic window. This is most likely a result of its intrinsic electrophilic character, which may push for nonspecific reactivity with biomolecules within cells. Its electrophilic character may also strongly contribute to its off-target toxicity. The highly reactive 1,4-dicarbonyl motif is able to form covalent adducts with nucleophilic residues, like primary amines and thiols. This has the potential to disrupt membrane lipids and proteins past deliberate targets. Basic cellular functions may be impaired by this limited selectivity, and the prediction of safety margins may become complicated. These disadvantages are still poorly charcterised in vivo, which limits current evaluation of safety, selectivity and clinical viability. Assessing if strong in vitro effects can change into effective in vivo exposures without this information is hypothetical at best.
Figure 7. Mechanistic strengths, context dependence, and translational challenges of Ophiobolin A. Membrane- and mitochondria-based mechanisms support non-apoptotic cancer cell killing but continue to be highly context-dependent, collectively revealing toxicity and pharmacokinetic limitations that encourage targeted, chemistry- and biology-guided translational strategies. Created in BioRender. Wilk, I. (2026) https://BioRender.com/ao6hz9a.

8.4. Future Directions for Medicinal and Translational Development

The OpA scaffold presents opportunities for medicinal chemistry optimisation from a drug development perspective. For example, semi-synthetic alterations led by pharmacophore-directed retrosynthesis have produced simplified bicyclic derivatives with preserved anticancer activity, demonstrating that structural complexity and electrophilic warheads can be adjusted to control effectiveness and selectivity [38]. SAR studies should be integrated with rigorous absorption, distribution, metabolism, and excretion (ADME) characterisation in future work to identify derivatives with improved safety and pharmacological properties. Emerging research directions expand the relevance of OpA beyond classical cytotoxicity. Systemic evaluation of lipid peroxidation data, iron dependency, and interaction with redox signalling systems would help to explain how OpA and its analogues activate these mechanisms and whether they can be used advantageously in precision oncology, given the growing attention around ferroptosis and other non-apoptotic death pathways as therapeutic targets [108]. In summary, OpA displays interesting mechanistic delivery and anticancer activity in cell-based models. However, addressing current gaps in in vivo validation, pharmacokinetic interpretation, and focused medicinal chemistry optimisation will be necessary to advance OpA toward therapeutic application.

Author Contributions

Conceptualisation, D.A., I.W. and D.B.-A.; methodology, D.A., I.W. and D.B.-A.; software, D.A., I.W. and D.B.-A.; validation, D.A., I.W. and D.B.-A.; formal analysis, D.A., I.W. and D.B.-A.; investigation, D.A., I.W. and D.B.-A.; resources, D.A., I.W. and D.B.-A.; data curation, D.A., I.W. and D.B.-A.; writing—original draft preparation, D.A., I.W. and D.B.-A.; writing—review and editing, D.A., I.W. and D.B.-A.; visualisation, D.A., I.W. and D.B.-A.; supervision, D.A., I.W. and D.B.-A.; project administration, D.A., I.W. and D.B.-A.; funding acquisition, D.A., I.W. and D.B.-A. All authors have read and agreed to the published version of the manuscript.

Funding

This research received no external funding.

Institutional Review Board Statement

Not applicable.

Data Availability Statement

No new data were created.

Acknowledgments

During the preparation of this manuscript/study, the author(s) used Grammarly (https://app.grammarly.com/ accessed on 29 March 2026) for the purposes of better grammar and enhancing overall clarity. The authors have reviewed and edited the output and take full responsibility for the content of this publication.

Conflicts of Interest

The authors declare no conflicts of interest.

Abbreviations

The following abbreviations are used in this manuscript:
ADMEAbsorption, distribution, metabolism, and excretion
ADCAntibody–drug conjugate
Akt Protein kinase B
AIP-1/AlixApoptosis-inducing protein 1
ATPAdenosine triphosphate
BGCBiosynthetic gene cluster
BKCaLarge-conductance Ca2+-activated potassium channel
Ca2+Calcium ion
CaMCalmodulin
CDKCyclin-dependent kinase
CHOPC/EBP homologous protein
COXCytochrome c oxidase (mitochondrial complex IV)
COX-2Cyclooxygenase-2
COX5ACytochrome c oxidase subunit 5A
CSCCancer stem cell
ΔΨmMitochondrial membrane potential
EMTEpithelial–mesenchymal transition
EREndoplasmic reticulum
ERKExtracellular signal-regulated kinase
EPREnhanced permeability and retention
FADFlavin adenine dinucleotide
GBMGlioblastoma
GFPPGeranylfarnesyl diphosphate
GI50Concentration causing 50% growth inhibition
GPX4Glutathione peroxidase 4
GSHReduced glutathione
HIGD2AHypoxia-inducible gene domain family member 2A
iNOSInducible nitric oxide synthase
IC50Half-maximal inhibitory concentration
JNKc-Jun N-terminal kinase
LC–MS/MSLiquid chromatography–tandem mass spectrometry
LPSLipopolysaccharide
MAPKMitogen-activated protein kinase
MICMinimum inhibitory concentration
mTORMechanistic target of rapamycin
MRSAMethicillin-resistant Staphylococcus aureus
MoAMechanism of action
NCCDNomenclature Committee on Cell Death
NONitric oxide
OpAOphiobolin A
OCROxygen consumption rate
P450Cytochrome P450 monooxygenase
PEPhosphatidylethanolamine
PI3KPhosphoinositide 3-kinase
PK Pharmacokinetics
PMCPubMed Central
RBRetinoblastoma protein
ROSReactive oxygen species
SARStructure–activity relationship
S6Ribosomal protein S6

References

  1. Newman, D.J.; Cragg, G.M. Natural Products as Sources of New Drugs over the Nearly Four Decades from 01/1981 to 09/2019. J. Nat. Prod. 2020, 83, 770–803. [Google Scholar] [CrossRef] [Scilit]
  2. Atanasov, A.G.; Zotchev, S.B.; Dirsch, V.M.; Supuran, C.T. Natural products in drug discovery: Advances and opportunities. Nat. Rev. Drug Discov. 2021, 20, 200–216. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  3. Deshmukh, S.K.; Prakash, V.; Ranjan, N. Marine Fungi: A Source of Potential Anticancer Compounds. Front. Microbiol. 2018, 8, 2536. [Google Scholar] [CrossRef] [Scilit]
  4. Nozoe, S.; Morisaki, M.; Tsuda, K.; Iitaka, Y.; Takahashi, N.; Tamura, S.; Ishibashi, K.; Shirasaka, M. The structure of ophiobolin, a C25 terpenoid having a novel skeleton. J. Am. Chem. Soc. 1965, 87, 4968–4970. [Google Scholar] [CrossRef] [Scilit]
  5. Au, T.K.; Chick, W.S.; Leung, P.C. The biology of ophiobolins. Life Sci. 2000, 67, 733–742. [Google Scholar] [CrossRef] [Scilit]
  6. Tian, W.; Deng, Z.; Hong, K. The Biological Activities of Sesterterpenoid-Type Ophiobolins. Mar. Drugs 2017, 15, 229. [Google Scholar] [CrossRef] [Scilit]
  7. Masi, M.; Dasari, R.; Evidente, A.; Mathieu, V.; Kornienko, A. Chemistry and biology of ophiobolin A and its congeners. Bioorg. Med. Chem. Lett. 2019, 29, 859–869. [Google Scholar] [CrossRef] [Scilit]
  8. Chai, H.; Yin, R.; Liu, Y.; Meng, H.; Zhou, X.; Zhou, G.; Bi, X.; Yang, X.; Zhu, T.; Zhu, W.; et al. Sesterterpene ophiobolin biosynthesis involving multiple gene clusters in Aspergillus ustus. Sci. Rep. 2016, 6, 27181. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  9. Leung, P.C.; Taylor, W.A.; Wang, J.H.; Tipton, C.L. Ophiobolin A. A natural product inhibitor of calmodulin. J. Biol. Chem. 1984, 259, 2742–2747. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  10. Leung, P.C.; Taylor, W.A.; Wang, J.H.; Tipton, C.L. Role of calmodulin inhibition in the mode of action of ophiobolin A. Plant Physiol. 1985, 77, 303–308. [Google Scholar] [CrossRef] [Scilit]
  11. Kong Au, T.; Chow Leung, P. Identification of the binding and inhibition sites in the calmodulin molecule for ophiobolin A by site-directed mutagenesis. Plant Physiol. 1998, 118, 965–973. [Google Scholar] [CrossRef] [Scilit]
  12. Gowans, F.A.; Thach, D.Q.; Wang, Y.; Altamirano Poblano, B.E.; Dovala, D.; Tallarico, J.A.; McKenna, J.M.; Schirle, M.; Maimone, T.J.; Nomura, D.K. Ophiobolin A covalently targets complex IV leading to mitochondrial metabolic collapse in cancer cells. ACS Chem. Biol. 2024, 19, 1260–1270. [Google Scholar] [CrossRef] [Scilit]
  13. Bury, M.; Girault, A.; Mégalizzi, V.; Spiegl-Kreinecker, S.; Mathieu, V.; Berger, W.; Evidente, A.; Kornienko, A.; Gailly, P.; Vandier, C.; et al. Ophiobolin A induces paraptosis-like cell death in human glioblastoma cells by decreasing BKCa channel activity. Cell Death Dis. 2013, 4, e561. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  14. Evidente, A. The incredible story of ophiobolin A and sphaeropsidin A: Two fungal terpenes from wilt-inducing phytotoxins to promising anticancer compounds. Nat. Prod. Rep. 2024, 41, 434–468. [Google Scholar] [CrossRef] [Scilit]
  15. Cai, R.; Jiang, H.; Mo, Y.; Guo, H.; Li, C.; Long, Y.; Zang, Z.; She, Z. Ophiobolin-Type Sesterterpenoids from the Mangrove Endophytic Fungus Aspergillus sp. ZJ-68. J. Nat. Prod. 2019, 82, 2268–2278. [Google Scholar] [CrossRef] [Scilit]
  16. Sugawara, F.; Strobel, G.; Strange, R.N.; Siedow, J.N.; Van Duyne, G.D.; Clardy, J. Phytotoxins from the pathogenic fungi Drechslera maydis and Drechslera sorghicola. Proc. Natl. Acad. Sci. USA 1987, 84, 3081–3085. [Google Scholar] [CrossRef] [Scilit]
  17. Zhao, X.L.; Niu, Y.C.; Deng, H.; Luo, D.Q. Characterization and phytotoxicity of ophiobolins produced by Bipolaris setariae. Mycoscience 2021, 62, 64–70. [Google Scholar] [CrossRef] [Scilit]
  18. Yuan, W.; Lv, S.; Chen, L.; Zhao, Y.; Deng, Z.; Hong, K. Production of sesterterpene ophiobolin by a bifunctional terpene synthase in Escherichia coli. Appl. Microbiol. Biotechnol. 2019, 103, 8785–8797. [Google Scholar] [CrossRef] [Scilit]
  19. Sohsomboon, N.; Kanzaki, H.; Nitoda, T. Unique antimicrobial spectrum of ophiobolin K produced by Aspergillus ustus. Biosci. Biotechnol. Biochem. 2018, 82, 422–424. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  20. Bury, M.; Novo-Uzal, E.; Andolfi, A.; Cimini, S.; Wauthoz, N.; Heffeter, P.; Lallemand, B.; Avolio, F.; Delporte, C.; Cimmino, A.; et al. Ophiobolin A, a sesterterpenoid fungal phytotoxin, displays higher in vitro growth-inhibitory effects in mammalian than in plant cells and displays in vivo antitumor activity. Int. J. Oncol. 2013, 43, 575–585. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  21. Zhang, C.; Wu, J.; Sun, Q.; Ding, S.; Tao, H.; He, Y.; Qiu, H.; Shu, B.; Zhu, D.; Zhu, H.; et al. De novo production of bioactive sesterterpenoid ophiobolins in Saccharomyces cerevisiae cell factories. Microb. Cell Fact. 2024, 23, 129. [Google Scholar] [CrossRef] [Scilit]
  22. Chidley, C.; Trauger, S.A.; Birsoy, K.; O’Shea, E.K. The anticancer natural product ophiobolin A induces cytotoxicity by covalent modification of phosphatidylethanolamine. eLife 2016, 5, e14601. [Google Scholar] [CrossRef] [Scilit]
  23. Aroujo, J.; Parker, H.; Boari, A.; Mason, E.; Otakpor, M.U.; Betancourt, T.; Kornienko, A.; Ciavatta, M.L.; Carbone, M.; Evidente, A.; et al. Derivatization of ophiobolin A and cytotoxicity toward breast and glioblastoma cancer stem cells: Varying the ketone and unsaturated aldehyde moieties. Bioorg. Med. Chem. Lett. 2025, 120, 130112. [Google Scholar] [CrossRef] [Scilit]
  24. Tsuna, K.; Noguchi, N.; Nakada, M. Convergent total synthesis of (+)-ophiobolin A. Angew. Chem. Int. Ed. 2011, 50, 9452–9455. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  25. Maslivetc, V.A.; Nabiul Hasan, M.; Boari, A.; Zejnelovski, A.; Evidente, A.; Sun, D.; Kornienko, A. Ophiobolin A derivatives with enhanced activities under tumor-relevant acidic conditions. Bioorg. Med. Chem. Lett. 2024, 110, 129863. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  26. Hue, Y.; Nam, Y.; Choi, B.; Kim, S.; Jang, S.H.; Chung, H.; Park, S.Y.; Kim, K.T. Comparative Genomics Reveals Conserved Ophiobolin Biosynthetic Gene Cluster and Necrotrophic Adaptation in Bipolaris oryzae. Plant Pathol. J. 2025, 41, 682–698. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  27. Ojo, O.; Njanje, I.; Abdissa, D.; Swart, T.; Higgitt, R.L.; Dorrington, R.A. Newly isolated terpenoids (covering 2019–2024) from Aspergillus species and their potential for the discovery of novel antimicrobials. Nat. Prod. Bioprospect. 2025, 15, 19. [Google Scholar] [CrossRef] [Scilit]
  28. Yan, J.; Pang, J.; Liang, J.; Yu, W.; Liao, X.; Aobulikasimu, A.; Yi, X.; Yin, Y.; Deng, Z.; Hong, K. The Biosynthesis and Transport of Ophiobolins in Aspergillus ustus 094102. Int. J. Mol. Sci. 2022, 23, 1903. [Google Scholar] [CrossRef] [Scilit]
  29. Fanelli, F.; Reveglia, P.; Masi, M.; Mulè, G.; Zonno, M.C.; Cimmino, A.; Vurro, M.; Evidente, A. Influence of light on the biosynthesis of ophiobolin A by Bipolaris maydis. Nat. Prod. Res. 2017, 31, 909–917. [Google Scholar] [CrossRef] [Scilit]
  30. Tsuna, K.; Noguchi, N.; Nakada, M. Enantioselective total synthesis of (+)-ophiobolin A. Chem. Eur. J. 2013, 19, 5476–5486. [Google Scholar] [CrossRef] [Scilit]
  31. Thach, D.Q.; Brill, Z.G.; Grover, H.K.; Esguerra, K.V.; Thompson, J.K.; Maimone, T.J. Total Synthesis of (+)-6-epi-Ophiobolin A. Angew. Chem. Int. Ed. 2020, 59, 1532–1536. [Google Scholar] [CrossRef] [Scilit]
  32. Dauben, W.G.; Hart, D.J. A synthesis of the ophiobolin nucleus. J. Org. Chem. 1977, 42, 922–923. [Google Scholar] [CrossRef] [Scilit]
  33. Brill, Z.G.; Grover, H.K.; Maimone, T.J. Enantioselective synthesis of an ophiobolin sesterterpene via a programmed radical cascade. Science 2016, 352, 1078–1082. [Google Scholar] [CrossRef] [Scilit]
  34. Vale, N.; Ferreira, A.; Matos, J.; Fresco, P.; Gouveia, M.J. Amino Acids in the Development of Prodrugs. Molecules 2018, 23, 2318. [Google Scholar] [CrossRef] [Scilit]
  35. Maslivetc, V.; Laguera, B.; Chandra, S.; Dasari, R.; Olivier, W.J.; Smith, J.A.; Bissember, A.C.; Masi, M.; Evidente, A.; Mathieu, V.; et al. Polygodial and Ophiobolin A Analogues for Covalent Crosslinking of Anticancer Targets. Int. J. Mol. Sci. 2021, 22, 11256. [Google Scholar] [CrossRef] [Scilit]
  36. Dasari, R.; Masi, M.; Lisy, R.; Ferdérin, M.; English, L.R.; Cimmino, A.; Mathieu, V.; Brenner, A.J.; Kuhn, J.G.; Whitten, S.T.; et al. Fungal metabolite ophiobolin A as a promising anti-glioma agent: In vivo evaluation, structure-activity relationship and unique pyrrolylation of primary amines. Bioorg. Med. Chem. Lett. 2015, 25, 4544–4548. [Google Scholar] [CrossRef] [Scilit]
  37. Zhang, C.; Liu, Y. Targeting cancer with sesterterpenoids: The new potential antitumor drugs. J. Nat. Med. 2015, 69, 255–266. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  38. Tao, Y.; Reisenauer, K.N.; Masi, M.; Evidente, A.; Taube, J.H.; Romo, D. Pharmacophore-Directed Retrosynthesis Applied to Ophiobolin A: Simplified Bicyclic Derivatives Displaying Anticancer Activity. Org. Lett. 2020, 22, 8307–8312. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  39. Kim, I.Y.; Kwon, M.; Choi, M.K.; Lee, D.; Lee, D.M.; Seo, M.J.; Choi, K.S. Ophiobolin A kills human glioblastoma cells by inducing endoplasmic reticulum stress via disruption of thiol proteostasis. Oncotarget 2017, 8, 106740–106752. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  40. Morrison, R.; Lodge, T.; Evidente, A.; Kiss, R.; Townley, H. Ophiobolin A, a sesterpenoid fungal phytotoxin, displays different mechanisms of cell death in mammalian cells depending upon the cancer cell origin. Int. J. Oncol. 2017, 50, 773–786. [Google Scholar] [CrossRef] [Scilit]
  41. Wang, Q.X.; Yang, J.L.; Qi, Q.Y.; Bao, L.; Yang, X.L.; Liu, M.M.; Huang, P.; Zhang, L.X.; Chen, J.L.; Cai, L.; et al. 3-Anhydro-6-hydroxy-ophiobolin A, a new sesterterpene inhibiting the growth of methicillin-resistant Staphylococcus aureus and inducing the cell death by apoptosis on K562, from the phytopathogenic fungus Bipolaris oryzae. Bioorg. Med. Chem. Lett. 2013, 23, 3547–3550. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  42. Van Puyenbroeck, V.; Vermeire, K. Inhibitors of protein translocation across membranes of the secretory pathway: Novel antimicrobial and anticancer agents. Cell. Mol. Life Sci. 2018, 75, 1541–1558. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  43. Desrivières, S.; Cooke, F.T.; Morales-Johansson, H.; Parker, P.J.; Hall, M.N. Calmodulin controls organization of the actin cytoskeleton via regulation of phosphatidylinositol (4,5)-bisphosphate synthesis in Saccharomyces cerevisiae. Biochem. J. 2002, 366, 945–951. [Google Scholar] [CrossRef] [Scilit]
  44. Hong, F.; Haldeman, B.D.; Jackson, D.; Carter, M.; Baker, J.E.; Cremo, C.R. Biochemistry of smooth muscle myosin light chain kinase. Arch. Biochem. Biophys. 2011, 510, 135–146. [Google Scholar] [CrossRef] [Scilit]
  45. Tan, L.T.; Chan, K.G.; Pusparajah, P.; Lee, W.L.; Chuah, L.H.; Khan, T.M.; Lee, L.H.; Goh, B.H. Targeting Membrane Lipid a Potential Cancer Cure? Front. Pharmacol. 2017, 8, 12. [Google Scholar]
  46. Rodolfo, C.; Rocco, M.; Cattaneo, L.; Tartaglia, M.; Sassi, M.; Aducci, P.; Scaloni, A.; Camoni, L.; Marra, M. Ophiobolin A Induces Autophagy and Activates the Mitochondrial Pathway of Apoptosis in Human Melanoma Cells. PLoS ONE 2016, 11, e0167672. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  47. Bladt, T.T.; Dürr, C.; Knudsen, P.B.; Kildgaard, S.; Frisvad, J.C.; Gotfredsen, C.H.; Seiffert, M.; Larsen, T.O. Bio-activity and dereplication-based discovery of ophiobolins and other fungal secondary metabolites targeting leukemia cells. Molecules 2013, 18, 14629–14650. [Google Scholar] [CrossRef] [Scilit]
  48. Yang, T.; Lu, Z.; Meng, L.; Wei, S.; Hong, K.; Zhu, W.; Huang, C. The novel agent ophiobolin O induces apoptosis and cell cycle arrest of MCF-7 cells through activation of MAPK signaling pathways. Bioorg. Med. Chem. Lett. 2012, 22, 579–585. [Google Scholar] [CrossRef] [Scilit]
  49. Lv, C.; Qin, W.; Zhu, T.; Wei, S.; Hong, K.; Zhu, W.; Chen, R.; Huang, C. Ophiobolin O isolated from Aspergillus ustus induces G1 arrest of MCF-7 cells through interaction with AKT/GSK3β/cyclin D1 signaling. Mar. Drugs 2015, 13, 431–443. [Google Scholar] [CrossRef] [Scilit]
  50. Sun, W.; Lv, C.; Zhu, T.; Yang, X.; Wei, S.; Sun, J.; Hong, K.; Zhu, W.; Huang, C. Ophiobolin-O reverses adriamycin resistance via cell cycle arrest and apoptosis sensitization in adriamycin-resistant human breast carcinoma (MCF-7/ADR) cells. Mar. Drugs 2013, 11, 4570–4584. [Google Scholar] [CrossRef] [Scilit]
  51. Al-Madhagi, H. Natural products-induced cancer cell paraptosis. Food Sci. Nutr. 2024, 12, 9866–9871. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  52. Sperandio, S.; Poksay, K.; de Belle, I.; Lafuente, M.J.; Liu, B.; Nasir, J.; Bredesen, D.E. Paraptosis: Mediation by MAP kinases and inhibition by AIP-1/Alix. Cell Death Differ. 2004, 11, 1066–1075. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  53. Ron, D.; Walter, P. Signal integration in the endoplasmic reticulum unfolded protein response. Nat. Rev. Mol. Cell Biol. 2007, 8, 519–529. [Google Scholar] [CrossRef] [Scilit]
  54. Bayir, H.; Kagan, V.E. Bench-to-bedside review: Mitochondrial injury, oxidative stress and apoptosis--there is nothing more practical than a good theory. Crit. Care 2008, 12, 206. [Google Scholar] [CrossRef] [Scilit]
  55. Dixon, S.J.; Lemberg, K.M.; Lamprecht, M.R.; Skouta, R.; Zaitsev, E.M.; Gleason, C.E.; Patel, D.N.; Bauer, A.J.; Cantley, A.M.; Yang, W.S.; et al. Ferroptosis: An iron-dependent form of nonapoptotic cell death. Cell 2012, 149, 1060–1072. [Google Scholar] [CrossRef] [Scilit]
  56. Yang, W.S.; SriRamaratnam, R.; Welsch, M.E.; Shimada, K.; Skouta, R.; Viswanathan, V.S.; Cheah, J.H.; Clemons, P.A.; Shamji, A.F.; Clish, C.B.; et al. Regulation of ferroptotic cancer cell death by GPX4. Cell 2014, 156, 317–331. [Google Scholar] [CrossRef] [Scilit]
  57. Su, L.J.; Zhang, J.H.; Gomez, H.; Murugan, R.; Hong, X.; Xu, D.; Jiang, F.; Peng, Z.Y. Reactive Oxygen Species-Induced Lipid Peroxidation in Apoptosis, Autophagy, and Ferroptosis. Oxid. Med. Cell. Longev. 2019, 2019, 5080843. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  58. Reisenauer, K.N.; Tao, Y.; Das, P.; Song, S.; Svatek, H.; Patel, S.D.; Mikhail, S.; Ingros, A.; Sheesley, P.; Masi, M.; et al. Epithelial-mesenchymal transition sensitizes breast cancer cells to cell death via the fungus-derived sesterterpenoid ophiobolin A. Sci. Rep. 2021, 11, 10652. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  59. Galluzzi, L.; Vitale, I.; Aaronson, S.A.; Abrams, J.M.; Adam, D.; Agostinis, P.; Alnemri, E.S.; Altucci, L.; Amelio, I.; Andrews, D.W.; et al. Molecular mechanisms of cell death: Recommendations of the Nomenclature Committee on Cell Death 2018. Cell Death Differ. 2018, 25, 486–541. [Google Scholar] [CrossRef] [Scilit]
  60. Bhatia, D.R.; Dhar, P.; Mutalik, V.; Deshmukh, S.K.; Verekar, S.A.; Desai, D.C.; Kshirsagar, R.; Thiagarajan, P.; Agarwal, V. Anticancer activity of Ophiobolin A, isolated from the endophytic fungus Bipolaris setariae. Nat. Prod. Res. 2016, 30, 1455–1458. [Google Scholar] [CrossRef] [Scilit]
  61. Hemmings, B.A.; Restuccia, D.F. PI3K-PKB/Akt pathway. Cold Spring Harb. Perspect. Biol. 2012, 4, a011189. [Google Scholar] [CrossRef] [Scilit]
  62. Johnson, G.L.; Lapadat, R. Mitogen-activated protein kinase pathways mediated by ERK, JNK, and p38 protein kinases. Science 2002, 298, 1911–1912. [Google Scholar] [CrossRef] [Scilit]
  63. Pakos-Zebrucka, K.; Koryga, I.; Mnich, K.; Ljujic, M.; Samali, A.; Gorman, A.M. The integrated stress response. EMBO Rep. 2016, 17, 1374–1395. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  64. Gomes, N.G.; Lefranc, F.; Kijjoa, A.; Kiss, R. Can Some Marine-Derived Fungal Metabolites Become Actual Anticancer Agents? Mar. Drugs 2015, 13, 3950–3991. [Google Scholar]
  65. Villalobo, A.; Berchtold, M.W. The Role of Calmodulin in Tumor Cell Migration, Invasiveness, and Metastasis. Int. J. Mol. Sci. 2020, 21, 765. [Google Scholar] [CrossRef] [Scilit]
  66. Linxweiler, M.; Schorr, S.; Schäuble, N.; Jung, M.; Linxweiler, J.; Langer, F.; Schäfers, H.J.; Cavalié, A.; Zimmermann, R.; Greiner, M. Targeting cell migration and the endoplasmic reticulum stress response with calmodulin antagonists: A clinically tested small molecule phenocopy of SEC62 gene silencing in human tumor cells. BMC Cancer 2013, 13, 574. [Google Scholar] [CrossRef] [Scilit]
  67. Okutachi, S.; Manoharan, G.B.; Kiriazis, A.; Laurini, C.; Catillon, M.; McCormick, F.; Yli-Kauhaluoma, J.; Abankwa, D. A Covalent Calmodulin Inhibitor as a Tool to Study Cellular Mechanisms of K-Ras-Driven Stemness. Front. Cell Dev. Biol. 2021, 9, 665673. [Google Scholar] [CrossRef] [Scilit]
  68. Stewart, T.A.; Yapa, K.T.; Monteith, G.R. Altered calcium signaling in cancer cells. Biochim. Biophys. Acta 2015, 1848, 2502–2511. [Google Scholar] [CrossRef] [Scilit]
  69. Au, T.K.; Chick, W.S.H.; Leung, P.C. Initial kinetics of the inactivation of calmodulin by the fungal toxin ophiobolin A. Int. J. Biochem. Cell Biol. 2000, 32, 1173–1182. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  70. Morrison, R.; Gardiner, C.; Evidente, A.; Kiss, R.; Townley, H. Incorporation of ophiobolin A into novel chemoembolization particles for cancer cell treatment. Pharm. Res. 2014, 31, 2904–2917. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  71. Ding, M.; He, M.; Li, D.; Ding, S.; Dong, C.; Zhao, H.; Song, H.; Hong, K.; Zhu, H. A Marine-Derived Small Molecule Inhibits Prostate Cancer Growth by Promoting Endoplasmic Reticulum Stress Induced Apoptosis and Autophagy. Phytother. Res. 2024, 38, 6004–6022. [Google Scholar] [CrossRef] [Scilit]
  72. Choi, B.K.; Trinh, P.T.H.; Lee, H.S.; Choi, B.W.; Kang, J.S.; Ngoc, N.T.D.; Van, T.T.T.; Shin, H.J. New Ophiobolin Derivatives from the Marine Fungus Aspergillus flocculosus and Their Cytotoxicities against Cancer Cells. Mar. Drugs 2019, 17, 346. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  73. Wang, Q.X.; Bao, L.; Yang, X.L.; Liu, D.L.; Guo, H.; Dai, H.Q.; Song, F.H.; Zhang, L.X.; Guo, L.D.; Li, S.J.; et al. Ophiobolins P–T, Five New Cytotoxic and Antibacterial Sesterterpenes from the Endolichenic Fungus Ulocladium sp. Fitoterapia 2013, 90, 220–227. [Google Scholar] [CrossRef] [Scilit]
  74. de Carvalho, C.R.; Vieira, M.d.L.; Cantrell, C.L.; Wedge, D.E.; Alves, T.M.; Zani, C.L.; Pimenta, R.S.; Sales Junior, P.A.; Murta, S.M.; Romanha, A.J.; et al. Biological Activities of Ophiobolin K and 6-epi-Ophiobolin K Produced by the Endophytic Fungus Aspergillus calidoustus. Nat. Prod. Res. 2016, 30, 478–481. [Google Scholar] [CrossRef] [Scilit]
  75. Zatout, R.; Masi, M.; Sangermano, F.; Vurro, M.; Zonno, M.C.; Santoro, E.; Calabrò, V.; Superchi, S.; Evidente, A. Drophiobiolins A and B, Bioactive Ophiobolan Sestertepenoids Produced by Dreschslera gigantea. J. Nat. Prod. 2020, 83, 3387–3396. [Google Scholar] [CrossRef] [Scilit]
  76. Liu, M.; Sun, W.; Shen, L.; Hao, X.; Al Anbari, W.H.; Lin, S.; Li, H.; Gao, W.; Wang, J.; Hu, Z.; et al. Bipolaricins A–I, Ophiobolin-Type Tetracyclic Sesterterpenes from a Phytopathogenic Bipolaris sp. Fungus. J. Nat. Prod. 2019, 82, 2897–2906. [Google Scholar] [CrossRef] [Scilit]
  77. Saito, N.; Mine, N.; Kufe, D.W.; Von Hoff, D.D.; Kawabe, T. CBP501 Inhibits EGF-Dependent Cell Migration, Invasion and Epithelial-to-Mesenchymal Transition of Non-Small Cell Lung Cancer Cells by Blocking KRas to Calmodulin Binding. Oncotarget 2017, 8, 74006–74018. [Google Scholar] [CrossRef] [Scilit]
  78. Krizsán, K.; Bencsik, O.; Nyilasi, I.; Galgóczy, L.; Vágvölgyi, C.; Papp, T. Effect of the Sesterterpene-Type Metabolites, Ophiobolins A and B, on Zygomycetes Fungi. FEMS Microbiol. Lett. 2010, 313, 135–140. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  79. Liu, M.T.; He, Y.; Shen, L.; Hu, Z.X.; Zhang, Y.H. Bipolarins A–H, Eight New Ophiobolin-Type Sesterterpenes with Antimicrobial Activity from Fungus Bipolaris sp. TJ403-B1. Chin. J. Nat. Med. 2019, 17, 935–944. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  80. Zhou, G.J.; Xiong, W.J.; Xu, W.; Dou, Z.R.; Liu, B.C.; Li, X.L.; Du, H.; Li, H.F.; Zhang, Y.Z.; Jiang, B.; et al. Diversity and Anti-Infectious Components of Cultivable Rhizosphere Fungi Derived from Three Species of Astragalus Plants in Northwestern Yunnan, China. J. Fungi 2024, 10, 736. [Google Scholar] [CrossRef] [Scilit]
  81. Arai, M.; Niikawa, H.; Kobayashi, M. Marine-Derived Fungal Sesterterpenes, Ophiobolins, Inhibit Biofilm Formation of Mycobacterium Species. J. Nat. Med. 2013, 67, 271–275. [Google Scholar] [CrossRef] [Scilit]
  82. Ding, W.; Uvarani, C.; Wang, F.; Xue, Y.; Wu, N.; He, L.; Tian, D.; Chen, M.; Zhang, Y.; Hong, K.; et al. New Ophiobolins from the Deep-Sea Derived Fungus Aspergillus sp. WHU0154 and Their Anti-Inflammatory Effects. Mar. Drugs 2020, 18, 575. [Google Scholar] [CrossRef] [Scilit]
  83. Zhang, Y.; Liu, H.; Chen, Y.; Lu, X.; Liu, Z.; Tan, H.; Zhang, W. Cyophiobiolins A–D, Ophiobolin Sestertepenoids from Cytospora rhizophorae. Phytochemistry 2022, 203, 113352. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  84. Leung, P.C.; Graves, L.M.; Tipton, C.L. Characterization of the Interaction of Ophiobolin A and Calmodulin. Int. J. Biochem. 1988, 20, 1351–1359. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  85. Solà, C.; Barrón, S.; Tusell, J.M.; Serratosa, J. The Ca2+/Calmodulin System in Neuronal Hyperexcitability. Int. J. Biochem. Cell Biol. 2001, 33, 439–455. [Google Scholar] [CrossRef] [Scilit]
  86. Najumudeen, A.K.; Jaiswal, A.; Lectez, B.; Oetken-Lindholm, C.; Guzmán, C.; Siljamäki, E.; Posada, I.M.; Lacey, E.; Aittokallio, T.; Abankwa, D. Cancer Stem Cell Drugs Target K-Ras Signaling in a Stemness Context. Oncogene 2016, 35, 5248–5262. [Google Scholar] [CrossRef] [Scilit]
  87. Kornienko, A.; La Clair, J.J. Covalent Modification of Biological Targets with Natural Products through Paal-Knorr Pyrrole Formation. Nat. Prod. Rep. 2017, 34, 1051–1060. [Google Scholar] [CrossRef] [Scilit]
  88. Manoharan, G.B.; Laurini, C.; Bottone, S.; Ben Fredj, N.; Abankwa, D.K. K-Ras Binds Calmodulin-Related Centrin1 with Potential Implications for K-Ras Driven Cancer Cell Stemness. Cancers 2023, 15, 3087. [Google Scholar] [CrossRef] [Scilit]
  89. Bencsik, O.; Papp, T.; Berta, M.; Zana, A.; Forgó, P.; Dombi, G.; Andersson, M.A.; Salkinoja-Salonen, M.; Vágvölgyi, C.; Szekeres, A. Ophiobolin A from Bipolaris oryzae Perturbs Motility and Membrane Integrities of Porcine Sperm and Induces Cell Death on Mammalian Somatic Cell Lines. Toxins 2014, 6, 2857–2871. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  90. Shen, L.; Liu, M.; He, Y.; Al Anbari, W.H.; Li, H.; Lin, S.; Chai, C.; Wang, J.; Hu, Z.; Zhang, Y. Novel Antimicrobial Compounds as Ophiobolin-Type Sesterterpenes and Pimarane-Type Diterpene from Bipolaris Species TJ403-B1. Front. Microbiol. 2020, 11, 856. [Google Scholar] [CrossRef] [Scilit]
  91. Parker, H.N.; Tao, Y.; Tobin, J.; Haberman, K.L.; Davis, S.; York, E.; Martinez, A.; Matsumoto, N.; Aroujo, J.; Park, J.H.; et al. Ophiobolin A Impacts Mitochondrial Redox Biology in an Epithelial-Mesenchymal Transition (EMT)-Specific Manner. Cancer Cell Int. 2026, 26, 80. [Google Scholar] [CrossRef] [Scilit]
  92. Boike, L.; Henning, N.J.; Nomura, D.K. Advances in Covalent Drug Discovery. Nat. Rev. Drug Discov. 2022, 21, 881–898. [Google Scholar] [CrossRef] [Scilit]
  93. Jackson, P.A.; Widen, J.C.; Harki, D.A.; Brummond, K.M. Covalent Modifiers: A Chemical Perspective on the Reactivity of α,β-Unsaturated Carbonyls with Thiols via Hetero-Michael Addition Reactions. J. Med. Chem. 2017, 60, 839–885. [Google Scholar] [CrossRef] [Scilit]
  94. McAulay, K.; Bilsland, A.; Bon, M. Reactivity of Covalent Fragments and Their Role in Fragment Based Drug Discovery. Pharmaceuticals 2022, 15, 1366. [Google Scholar] [CrossRef] [Scilit]
  95. Grimsrud, P.A.; Xie, H.; Griffin, T.J.; Bernlohr, D.A. Oxidative Stress and Covalent Modification of Protein with Bioactive Aldehydes. J. Biol. Chem. 2008, 283, 21837–21841. [Google Scholar] [CrossRef] [Scilit]
  96. Pósa, A.; Szabó, R.; Szalai, Z.; Kupai, K.; Deim, Z.; Murlasits, Z.; Bencsik, O.; Szekeres, A.; Vágvölgyi, C.; Balogh, L.; et al. The Effect of Acute Ophiobolin A Treatment on HO-Mediated Inflammatory Processes. Hum. Exp. Toxicol. 2017, 36, 594–602. [Google Scholar] [CrossRef] [Scilit]
  97. Bulbake, U.; Doppalapudi, S.; Kommineni, N.; Khan, W. Liposomal Formulations in Clinical Use: An Updated Review. Pharmaceutics 2017, 9, 12. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  98. Choi, J.W.; Cho, H.J.; Park, J.H.; Baek, S.Y.; Chung, J.W.; Kim, D.D.; Kim, H.C. Comparison of Drug Release and Pharmacokinetics after Transarterial Chemoembolization Using Diverse Lipiodol Emulsions and Drug-Eluting Beads. PLoS ONE 2014, 9, e115898. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  99. Tanaka, T.; Nishiofuku, H.; Hukuoka, Y.; Sato, T.; Masada, T.; Takano, M.; Gilbert, C.W.; Obayashi, C.; Kichikawa, K. Pharmacokinetics and Antitumor Efficacy of Chemoembolization Using 40 µm Irinotecan-Loaded Microspheres in a Rabbit Liver Tumor Model. J. Vasc. Interv. Radiol. 2014, 25, 1037–1044.e2. [Google Scholar] [CrossRef] [Scilit]
  100. Malagari, K.; Kiakidis, T.; Pomoni, M.; Moschouris, H.; Emmanouil, E.; Spiridopoulos, T.; Sotirchos, V.; Tandeles, S.; Koundouras, D.; Kelekis, A.; et al. Pharmacokinetics, Safety, and Efficacy of Chemoembolization with Doxorubicin-Loaded Tightly Calibrated Small Microspheres in Patients with Hepatocellular Carcinoma. Cardiovasc. Intervent. Radiol. 2016, 39, 1379–1391. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  101. Nsairat, H.; Khater, D.; Sayed, U.; Odeh, F.; Al Bawab, A.; Alshaer, W. Liposomes: Structure, Composition, Types, and Clinical Applications. Heliyon 2022, 8, e09394. [Google Scholar] [CrossRef] [Scilit]
  102. Sharmila, A.; Bhadra, P.; Kishore, C.; Selvaraj, C.I.; Kavalakatt, J.; Bishayee, A. Nanoformulated Terpenoids in Cancer: A Review of Therapeutic Applications, Mechanisms, and Challenges. Cancers 2025, 17, 3013. [Google Scholar] [CrossRef] [Scilit]
  103. Cheng, X.; Li, H.; Ge, X.; Chen, L.; Liu, Y.; Mao, W.; Zhao, B.; Yuan, W.E. Tumor-Microenvironment-Responsive Size-Shrinkable Drug-Delivery Nanosystems for Deepened Penetration into Tumors. Front. Mol. Biosci. 2020, 7, 576420. [Google Scholar] [CrossRef] [Scilit]
  104. Xing, J.; Lu, W.; Zhang, Y.; Yang, C.; Yang, J.; Shi, J.; Wang, Y. Design of Prodrugs with Reactive Oxygen Species as Activators and Their Application in Tumor Therapy. Theranostics 2026, 16, 1295–1327. [Google Scholar] [CrossRef] [Scilit]
  105. Shabat, D.; Rader, C.; List, B.; Lerner, R.A.; Barbas, C.F., 3rd. Multiple Event Activation of a Generic Prodrug Trigger by Antibody Catalysis. Proc. Natl. Acad. Sci. USA 1999, 96, 6925–6930. [Google Scholar] [CrossRef] [Scilit]
  106. Ranganathan, S.; Ojo, T.; Subramanian, A.; Tobin, J.; Kornienko, A.; Boari, A.; Evidente, A.; Benton, M.L.; Romo, D.; Taube, J.H. Gasdermin D Cleavage and Cytokine Release, Indicative of Pyroptotic Cell Death, Induced by Ophiobolin A in Breast Cancer Cell Lines. Int. J. Mol. Sci. 2026, 27, 618. [Google Scholar] [CrossRef] [Scilit]
  107. Evidente, A.; Kornienko, A.; Lefranc, F.; Cimmino, A.; Dasari, R.; Evidente, M.; Mathieu, V.; Kiss, R. Sesterterpenoids with Anticancer Activity. Curr. Med. Chem. 2015, 22, 3502–3522. [Google Scholar] [CrossRef] [Scilit]
  108. Ubellacker, J.M.; Dixon, S.J. Prospects for Ferroptosis Therapies in Cancer. Nat. Cancer 2025, 6, 1326–1336. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  109. Bebber, C.M.; Müller, F.; Prieto Clemente, L.; Weber, J.; von Karstedt, S. Ferroptosis in Cancer Cell Biology. Cancers 2020, 12, 164. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  110. Thi Nghiem, T.H.; Kusuma, F.; Park, J.; Joe, Y.; Chung, H.T.; Han, J. Brief guide to detecting ferroptosis. Mol. Cells 2025, 48, 100276. [Google Scholar] [CrossRef] [Scilit] [PubMed]
  111. Li, F.J.; Long, H.Z.; Zhou, Z.W.; Luo, H.Y.; Xu, S.G.; Gao, L.C. System Xc/GSH/GPX4 axis: An important antioxidant system for the ferroptosis in drug-resistant solid tumor therapy. Front. Pharmacol. 2022, 13, 910292. [Google Scholar] [CrossRef] [Scilit] [PubMed]
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