Home Journals Articles Updates About
CN
image
收藏切换
Tumor-Derived Exosomal Fatty Acids Reprogram Neutrophils to Drive Neutrophil Extracellular Traps Formation and Lung Cancer Progression
收藏切换
PDF
Lulu Han1, 2, 3, *, Yuxin Chen1, 2, 3, Ruchen Wu1, Junze Chen1, Zhaokai Chen1, Ying Cai1, Shuxin Huang1, Haoqing Gu1, Xiaoyi Zhuang1, Yanfang Lv1, Huizhong Li1, 2, 3, Liantao Li2, 3, *, Gang Wang1, 2, 3, *
Research. Vol 9 Article ID 1278
Less
收藏切换
Research. Vol 9 Article ID 1278
• RESEARCH ARTICLE •
Tumor-Derived Exosomal Fatty Acids Reprogram Neutrophils to Drive Neutrophil Extracellular Traps Formation and Lung Cancer Progression
Full
Lulu Han1, 2, 3, *, Yuxin Chen1, 2, 3, Ruchen Wu1, Junze Chen1, Zhaokai Chen1, Ying Cai1, Shuxin Huang1, Haoqing Gu1, Xiaoyi Zhuang1, Yanfang Lv1, Huizhong Li1, 2, 3, Liantao Li2, 3, *, Gang Wang1, 2, 3, *
Affiliations
  • 1Cancer Institute, Xuzhou Medical University, 209 Tongshan Road, Xuzhou 221004, China.
  • 2Center of Clinical Oncology, The Affiliated Hospital of Xuzhou Medical University, 99 West Huaihai Road, Xuzhou 221002, China.
  • 3Jiangsu Center for the Collaboration and Innovation of Cancer Biotherapy, Xuzhou Medical University, 209 Tongshan Road, Xuzhou 221004, China.
About Author:

† These authors contributed equally to this work.

Published: 2026-05-20 doi: 10.34133/research.1278
Outline
收藏切换

Tumor-infiltrating neutrophils are increasingly recognized as key drivers of cancer progression, but the mechanisms that govern their protumoral reprogramming remain elusive. Here, we demonstrated that lung cancer-derived exosomes (LDEs) deliver free fatty acids into neutrophils, triggering lipid accumulation, fatty acid β-oxidation, and mitochondrial reactive oxygen species production. This metabolic reprogramming culminates in enhanced neutrophil extracellular traps (NETs) formation, which accelerates lung cancer growth. Mechanistically, Ras-related protein Rab-34 (Rab34), a small guanosine triphosphatase, regulates neutrophil uptake of LDEs. Knockdown of Rab34 in neutrophils dramatically attenuated LDEs-induced lipid accumulation, fatty acid β-oxidation activation, and NETs formation, thereby mitigating neutrophil-involved lung cancer progression in vivo. Deoxyribonuclease I-mediated NETs degradation further confirmed the dependency of lung cancer growth on NETs. These findings uncovered a Rab34-dependent way by which LDEs reprogram neutrophils via exosomal free fatty acids, offering Rab34 and NET-associated pathways as potential therapeutic targets in lung cancer.

Lulu Han, Yuxin Chen, Ruchen Wu, Junze Chen, Zhaokai Chen, Ying Cai, Shuxin Huang, Haoqing Gu, Xiaoyi Zhuang, Yanfang Lv, Huizhong Li, Liantao Li, Gang Wang. Tumor-Derived Exosomal Fatty Acids Reprogram Neutrophils to Drive Neutrophil Extracellular Traps Formation and Lung Cancer Progression[J]. Research, 2026 , 9 (5) : 1278 - . DOI: 10.34133/research.1278
Full Text
Less
Introduction
Less
Lung cancer continues to be the primary cause of cancer-related mortality worldwide [1]. Although therapeutic approaches have advanced, their efficacy remains limited by the complex tumor microenvironment (TME), which facilitates tumor growth and angiogenesis while negatively modulating antitumor immunity [2]. Neutrophils constitute the predominant immune cell subpopulation in lung cancer TME [3,4]. Strikingly, numerous publications have shown that neutrophil depletion abrogates lung cancer growth in mice [5–7]. We and others have reported that tumor-infiltrating neutrophils mount a convergent reprogramming into a protumoral state, which fuels tumor progression [8–10]. However, the mechanisms driving this protumoral reprogramming are poorly defined.
Tumor-infiltrating neutrophils accelerate lung cancer progression by forming neutrophil extracellular traps (NETs) [11,12]. These web-like structures consist of DNA, myeloperoxidase (MPO), histones, and antimicrobial proteins [13], and they play a crucial role in combating pathogens. There is, however, growing consensus that NETs play a key role in facilitating cancer progression [14,15]. Inhibiting NETs formation or targeting their components is being explored as a potential therapeutic strategy in lung cancer treatment [11]. Elevated NETs level in cancer patients is correlated with metastasis and therapy resistance [16,17]. NETs triggered by tumor cells combines with integrin αvβ1 and matrix metalloproteinase-9 (MMP-9) to jointly activate transforming growth factor-β, leading to epithelial–mesenchymal transition of tumor cells and low chemotherapy efficacy [18]. Recently, our study found that lung cancer cells induced neutrophil activation and release of NETs-associated proteins, such as MMP-9, exacerbating lung cancer growth [10]. However, the mechanisms by which lung cancer cells trigger NETs formation remain poorly understood.
Tumor cells release soluble factors including exosomes, proteins, and lipids to communicate with various immune cells [19–21]. As nanoscale extracellular vesicles, tumor-associated exosomes are pivotal mediators of intercellular communication, especially in the TME [22]. These vesicles consist of a lipid bilayer encapsulating proteins, RNA, and lipids, which enables them to transfer bioactive molecules to various immune cells [22]. The lipid composition of exosomes influences their biophysical properties, such as membrane fluidity and stability, which in turn affect their interactions with recipient cells. In the context of immunity, tumor-derived exosomes employ immunosuppressive lipids to modulate immune cell function [4,22]. This not only impedes dendritic cell maturation, T cell activation, and proper macrophage polarization but also fosters an immunosuppressive microenvironment that fuels tumor progression [23,24]. Thus, understanding the specific roles of exosome lipids in mediating immune responses, particularly in relation to NETs formation, is crucial for developing therapeutic strategies aimed to reactivate antitumor immunity in lung cancer.
Here, we show that free fatty acid (FFA)-carrying exosomes from lung cancer cells (LDEs) reprogram neutrophils toward a protumoral state, equipping them with the capacity to produce NETs and promote tumor growth. Uptake of LDEs resulted in increased intracellular fatty acids and subsequently fatty acid β-oxidation (FAO), mitochondrial reactive oxygen species (mtROS) production, and thus NETs formation. Furthermore, the small guanosine triphosphatase (GTPase) protein Rab34 was identified as a critical regulator of exosome uptake in neutrophils. Hence, our findings revealed a mechanistic insight into neutrophil-mediated tumor progression and provided Rab34 and NET-associated pathways as potential therapeutic targets.
Results
Less
Exposure to lung cancer cells led to lipid accumulation of neutrophils
To investigate how lung cancer promotes neutrophil activation during tumor progression, we performed RNA sequencing (RNA-seq) of neutrophils exposed to lung cancer cell-conditioned medium (CM). Reactome enrichment analysis revealed that lung cancer-educated neutrophils up-regulated lipid metabolism-related genes, with a pronounced enrichment in lipid metabolic pathways compared to controls (Fig. 1A and B), suggesting enhanced lipid-handling capacity. Nile Red staining confirmed substantial lipid accumulation in tumor-infiltrating neutrophils sorted from mouse Lewis lung carcinoma (LLC) tumors, supporting these transcriptomic findings (Fig. 1C). To validate these observations, we incubated mouse bone marrow neutrophils (BMNs) and human neutrophil-like differentiated HL-60 (dHL-60) cells [25,26] with species-matched CM from either mouse (LLC) or human (A549) lung cancer cell lines. Nile Red staining intensity markedly increased in neutrophils cultured with lung cancer cell-CM compared to controls (Fig. 1D and E). In addition, neutrophils cultured with lung cancer cell-CM exhibit elevated lipid content, as clearly confirmed by BODIPY 493/503 fluorescence staining (Fig. 1F and G). These results demonstrated that lung cancer cells promoted lipid accumulation in neutrophils, suggesting that tumor-derived factors induce the formation of lipid-laden neutrophils both in vivo and in vitro.
Lung cancer cell-derived exosomes potentiated lipid accumulation in neutrophils, thereby boosting their protumoral function
Tumor cells communicate with various immune cells by releasing soluble factors such as proteins, lipids, and exosomes [19,20]. To identify the key mediators of neutrophil lipid accumulation, we fractionated lung cancer cell-CM via ultracentrifugation to obtain precipitated exosomes and exosome-free soluble medium. The isolated exosomes were characterized by nanoparticle tracking analysis (typical size ~100 nm), positive for the exosomal marker CD9 and negative for calnexin by western blot, and displayed a cup-shaped morphology by transmission electron microscopy (Fig. S1A to C). Nile Red staining revealed that lung cancer cell-derived exosomes induced lipid accumulation in neutrophils instead of exosome-free soluble medium (Fig. 2A and B), indicating their central role in this process. Consistent with this mechanism, GW4869, an inhibitor of exosome biogenesis that blocks neutral sphingomyelinase (nSMase) activity (Fig. S1D), markedly reduced lipid accumulation in neutrophils (Fig. 2C and D). We also performed short hairpin RNA (shRNA)-mediated knockdown of nSMase (SMPD2) in A549 lung cancer cells (Fig. S1E). Knockdown of nSMase markedly reduced exosome secretion (Fig. S1F). CM from nSMase-knockdown cancer cells failed to induce lipid accumulation in neutrophils (Fig. S1G), mirroring the effect of GW4869 treatment. These findings directly demonstrated that lung cancer cell-derived exosomes critically regulate neutrophil lipid accumulation.
To further investigate whether the lipid accumulation of neutrophils was resulted from the uptake of lung cancer cell-derived exosomes, green fluorescent protein (GFP)-labeled exosomes were generated and collected with CD9-GFP-transduced LLC cells (Fig. S1H to J). Then, neutrophils were cultured with or without LLC-CD9-GFP CM. The results indicated a time-dependent increase in GFP and Nile Red levels in BMNs (Fig. 2E and F). Furthermore, confocal microscopy revealed intracellular punctate fluorescence, confirming active uptake of exosomes by neutrophils (Fig. 2G). Next, we isolated exosomes from murine lung epithelial (MLE) and Beas2b cells, representing noncancerous mouse and human lung epithelial cell lines. Neither MLE- nor Beas2b-derived exosomes increased neutrophil lipid levels, demonstrating that lung cancer cell-derived exosomes uniquely induce lipid accumulation in neutrophils (Fig. 2H and I). Collectively, these data demonstrated that lung cancer cell-derived exosomes induce lipid accumulation in neutrophils.
We next assessed whether LDEs promote tumor progression through neutrophil reprogramming. In vitro, LLC or A549 cells cultured with CM from LDE-treated neutrophils exhibited markedly increased viability compared to cells cultured with medium from untreated neutrophils (Fig. 2J and K). In vivo, adoptive transfer of LDE-primed neutrophils into tumor-bearing mice obviously enhanced tumor growth (Fig. 2L to N). Collectively, these data demonstrated that LDEs reprogram neutrophils toward a protumoral phenotype that directly supports lung cancer cell growth both in vitro and in vivo.
Lung cancer cell-derived exosomes deliver FFAs into neutrophils to induce lipid accumulation
To determine which lipids contribute to the lipid accumulation of neutrophils, lipid metabolites in neutrophils were analyzed using high-performance liquid chromatography-tandem mass spectrometry (HPLC-MS/MS) after culturing with or without lung cancer cell-derived exosomes. Partial least-squares discriminant analysis of lipidomics data from BMNs exposed to LLC-exosomes revealed distinct metabolic clustering compared to control neutrophils (Fig. 3A). Variable importance in projection analysis identified FFAs as the primary metabolites driving this separation (Fig. 3B). Lipid heatmap confirmed elevated FFA levels in exosome-stimulated neutrophils (Fig. 3C), suggesting that FFAs from lung cancer cell-derived exosomes may promote lipid accumulation. Comparative analysis demonstrated markedly higher FFA levels in exosomes from lung cancer cells than in those from noncancerous Beas2b and MLE cell lines (Fig. 3D and Fig. S2A). Neutrophils cultured with lung cancer cell-derived exosomes exhibited corresponding increases in lipid accumulation (Fig. 3E and Fig. S2B).
To monitor the intercellular transport of FFAs between lung cancer cells and neutrophils, a fluorescent fatty acid analog BODIPYTM FL C16 (C16) was used in lung cancer cell culture (Fig. 3F). Neutrophils showed markedly enhanced C16 fluorescence after exposure to exosomes from LLC or A549 cells preincubated with C16 for 4 h (Fig. 3G to L). GW4869-treated cancer cell-CM partially reduced this fluorescence accumulation (Fig. 3M and N), confirming direct fatty acid transfer via exosomes.
To directly test whether exosomal FFAs derived from cancer cell lipid metabolism are critical for neutrophil reprogramming, we generated stable fatty acid synthase-knockdown (FASN-KD) LLC and A549 cell lines using shRNA (Fig. S2C). Under serum-starved conditions, exosomes isolated from FASN-KD cells (LDEs-FASN-KD) exhibited markedly reduced FFA content compared to control exosomes (Fig. S2D and E). Accordingly, neutrophils lipid accumulation was markedly reduced after treatment with LDEs-FASN-KD (Fig. S2F and G). These results demonstrated that cancer cell FFA loading into exosomes is essential for exosome-induced neutrophil reprogramming.
To assess whether lung cancer cell factors stimulate neutrophil lipid accumulation through endogenous fatty acid synthesis, FASN was inhibited with the inhibitor C75. Treatment with C75 failed to attenuate lipid accumulation induced by cancer cell-CM (Fig. 3O and P), excluding de novo synthesis as a major contributor in neutrophils. Although tumor-educated neutrophils transcriptionally up-regulate lipid metabolism pathways, their actual lipid accumulation stems largely from exosome-delivered FFAs, not from de novo synthesis. Collectively, these findings demonstrated that lipid buildup in neutrophils results primarily from uptake of FFAs delivered by lung cancer cell-derived exosomes rather than self-synthesis.
Lung cancer cell-derived exosomes promote neutrophil-induced tumor progression in a NETs-dependent manner
Our prior study demonstrated that tumor-educated neutrophils promote lung cancer progression through MMP-9 synthesis and release [10]. Given that MMP-9 is also a key component of NETs [27], we hypothesized that LDEs may drive tumor progression by inducing NETs formation. To test this, we first examined whether LDEs affect MMP-9 expression. Indeed, LDE-treated neutrophils showed increased MMP-9 levels (Fig. S3A and B), suggesting that exosomes may simultaneously prime neutrophils for both MMP-9 release and NETosis. We next assessed NETs formation directly. Neutrophils stimulated with LDEs exhibited marked increases in classic NETs markers, including MPO–DNA complexes, cell-free DNA (cfDNA), and citrullinated histone H3 (CitH3), compared to controls (Fig. 4A to F). Immunofluorescence staining confirmed the presence of extracellular DNA fibers, characteristic of NET release, in LDE-treated neutrophils, while control neutrophils retained intact nuclei (Fig. S3C and D). Furthermore, treating neutrophils with increasing concentrations of LDEs (0 to 80 μg/ml) resulted in a graded increase in MPO–DNA, cfDNA, and CitH3 levels, accompanied by progressive lipid accumulation (Fig. S3E to H). These dose-response data further support a causal relationship between exosome exposure and NETs induction. These findings establish a direct role for lung cancer cell-derived exosomes in inducing NETs formation.
To assess the effect of NETs on lung cancer cells, we incubated the cells with CM from neutrophils that had been treated with or without LDEs and with or without deoxyribonuclease I (DNase I), an enzyme that degrades NETs. Cell Counting Kit-8 assays revealed that CM from LDE-primed neutrophils markedly enhanced lung cancer cell viability, an effect that was abolished by DNase I cotreatment (Fig. S3I and J), confirming that NETs directly promote lung cancer cell proliferation in vitro. To investigate whether exosome-induced NETs causally contribute to tumor progression, we therapeutically administered DNase I intraperitoneally to mice bearing LLC tumors. In line with the in vitro data, exosome-primed neutrophils markedly increased tumor growth, resulting in greater tumor volume and weight (Fig. 4G to I). Strikingly, DNase I-mediated degradation of NETs blocked the ability of exosome-educated neutrophils to promote tumorigenesis (Fig. 4G to I). Immunofluorescence analysis of tumor tissues further corroborated these observations. Tumors from mice that received exosome-primed neutrophils exhibited robust NET formation, as evidenced by the characteristic localization and morphology of MPO and CitH3 (Fig. 4J). The NETs induced by LDEs were effectively eliminated by in vivo DNase I treatment (Fig. 4J). These results demonstrated that NETs are essential for lung cancer cell-derived exosome-primed neutrophil-driven tumor progression.
Lung cancer-derived exosomal fatty acids promote NETs formation through FAO pathways activation in neutrophils
To determine the contribution of exosomal fatty acids to NETs formation, we treated neutrophils with either LDEs or a combination of FFAs (palmitic, stearic, and oleic acid). Both treatments markedly induced NETs formation, as quantified by established NETs markers (Fig. 5A to F), demonstrating that exosome-derived fatty acids promote lipid accumulation in neutrophils, ultimately driving NETs formation. To determine whether specific fatty acid species differentially regulate NETosis, we treated neutrophils with individual FFAs, palmitic, stearic, or oleic acid. All 3 induced NETs formation and mtROS production comparable to the exosomes (Fig. S4A to D), demonstrating that both saturated and unsaturated FFAs drive NETosis. Crucially, the same FASN-KD LDEs failed to induce NETs formation. However, supplementing with exogenous FFAs completely restored their NETs-promoting effect (Fig. S5A to F). These results confirmed that the defective NETs induction stems specifically from the reduced FFA content in FASN-KD LDEs. To exclude a contribution from proteins, we heat-inactivated LDEs prior to neutrophil treatment. The heat-inactivated LDEs fully retained their ability to induce NETs formation (Fig. S5G to L), indicating that the NET-promoting activity is mediated by heat-stable components, primarily lipids, rather than protein cargo. Collectively, these findings establish that exosomal FFAs are both necessary and sufficient to drive NETs formation in neutrophils.
RNA-seq analysis revealed activation of FAO pathways in tumor-educated neutrophils (Fig. S5M). Subsequent quantitative real-time polymerase chain (PCR) analysis showed up-regulation of CPT1a, the rate-limiting enzyme for mitochondrial FAO, in exosome-treated neutrophils (Fig. 5G). To directly assess FAO flux, we measured the oxygen consumption rate (OCR) in BMNs treated with or without LDEs using a Seahorse analyzer. LDE treatment markedly increased both the basal and maximal OCRs. These increases were completely abolished by the CPT1a inhibitor etomoxir, confirming the specific activation of CPT1a-dependent FAO (Fig. S6A and B).
MS/MS analysis of neutrophil metabolites observed a marked remodeling of the carnitine pool, with reduced free carnitine and accumulation of long-chain species, including C16:0- and C18:1-carnitine (Fig. 5H), consistent with enhanced FAO flux. Western blot analysis confirmed CPT1a protein expression was increased following exosome treatment (Fig. 5I and J), indicating that exosomal fatty acids activate neutrophil FAO through CPT1a up-regulation.
Excessive FAO activation increases mitochondrial demand and mtROS production [28]. Consistent with this, MitoTracker and MitoSOX staining revealed elevated mitochondrial mass and mtROS levels in exosome-treated neutrophils (Fig. 5K to N). To determine whether FAO-driven mtROS contributes to NETs formation, CPT1a was inhibited with etomoxir during exosome exposure. Not surprising, etomoxir substantially suppressed exosome-induced NETs production (Fig. 5O to T). We further employed shRNA-mediated knockdown of CPT1a in HL-60-derived neutrophils. After confirming efficient CPT1a silencing at the protein level (Fig. S6C), we treated these cells with LDEs. The results aligned with our etomoxir data, demonstrating that CPT1a knockdown attenuated LDE-induced NETs formation (Fig. S6D to F). Similarly, the ROS scavenger N-acetylcysteine blocked NETs formation triggered by LDEs (Fig. S6G to L). These findings collectively indicate that FAO critically regulates NETs formation induced by exosomal fatty acids from lung cancer cells.
Rab34 mediates neutrophil uptake of LDEs to promote NETs formation and tumor progression
To identify key mediators of exosome internalization in neutrophils, we analyzed RNA-seq data and discovered that lung cancer cell-CM strongly up-regulated Rab34 (Fig. 6A), a small GTPase which reported in regulating vesicular trafficking [29–32]. Consistent with this, exosome treatment also markedly increased Rab34 expression in neutrophils (Fig. 6B and C). To determine whether Rab34 dominantly mediates the uptake of exosomes, shRNA-mediated knockdown of Rab34 was performed in HL-60-derived neutrophils (Fig. S7A). Rab34 deficiency substantially reduced both fluorescein isothiocyanate-exosome uptake and lipid accumulation (Fig. 6D and E), confirming its critical role in exosome internalization.
We next examined whether Rab34 mediates NETs formation upon exosome exposure. Rab34 knockdown prevented the exosome-induced increase in mitochondrial mass and mtROS (Fig. 6F and G) and markedly suppressed NETs formation (Fig. 6H to J). To determine whether Rab34 functions primarily in FFA delivery, we performed rescue and overexpression experiments. FFA supplementation fully restored NETs formation in Rab34-silenced neutrophils despite impaired exosome uptake (Fig. S7B to D), indicating that the downstream FAO–NETs axis remains intact when FFAs are supplied extracellularly. Conversely, Rab34 overexpression enhanced exosome uptake, lipid accumulation, and NETs formation (Fig. S7E to J). These results demonstrated that Rab34 is both necessary and sufficient for exosome uptake and subsequent neutrophil reprogramming.
However, the expression of NETs marker CitH3 was not affected by Rab34 depletion in lipopolysaccharide- or phorbol 12-myristate 13-acetate-stimulated neutrophils (Fig. S7K and L), suggesting that Rab34 specifically promotes NETs via regulating exosome uptake rather than neutrophil activation pathways.
To validate these findings in vivo, BMNs were pretreated with Rab34-small interfering RNA (siRNA) liposomes ex vivo and then injected into tumor-bearing mice, achieving selective Rab34 knockdown in tumor-infiltrating neutrophils but not macrophages (Fig. S7M and N). Using a murine lung cancer model coinjected with LLC cells and exosome-educated neutrophils, we demonstrated that Rab34 knockdown abrogated the tumor-promoting effects of these neutrophils (Fig. 6K to M). Furthermore, Rab34 knockdown markedly reduced lipid accumulation in tumor-infiltrating neutrophils and NETs formation in vivo (Fig. 6N and O). To validate our findings in a physiologically relevant setting, we established an orthotopic lung cancer model. Mice receiving control siRNA-treated BMNs exhibited obviously increased lung tumor burden, elevated intratumoral NETs formation, and more severe body weight loss. In contrast, Rab34 knockdown in neutrophils markedly attenuated all these parameters, confirming that Rab34-mediated exosome uptake drives lung cancer progression in the lung microenvironment (Fig. 6P to S). These findings definitively establish Rab34 as a critical mediator of exosome uptake in neutrophils and its essential role in promoting lung cancer progression.
Exosomal FFAs are required for neutrophil-mediated tumor promotion in vivo
To definitively establish that exosomal FFAs drive neutrophil-mediated tumor progression, we performed in vivo rescue experiments combining genetic and lipid supplementation strategies. Wild-type exosomes (LLCFASN-WT-EXOs) markedly promoted tumor growth, whereas FFA-deficient exosomes from FASN-KD cells (LLCFASN-KD-EXOs) lost this capacity. Strikingly, exogenous FFA supplementation fully restored the protumorigenic effect of FASN-KD exosomes, identifying FFAs as the critical cargo. Furthermore, Rab34 silencing in neutrophils abolished the tumor-promoting effect of wild-type exosomes, a defect partially rescued by exogenous FFAs (Fig. 7A to C). Consistently, intratumoral NETs formation, as measured by MPO–DNA levels, correlated with tumor growth across all groups, with the highest levels in FASN-WT and FFA-rescued groups and marked reduction upon Rab34 silencing (Fig. 7D). These findings establish a mechanistic axis: Cancer cell-derived exosomal FFAs, internalized via Rab34-dependent uptake, reprogram neutrophils to fuel lung cancer progression (Fig. 7E). This work positions exosomal lipid transfer as a key driver of tumor–immune crosstalk and highlights Rab34 and FAO as potential therapeutic targets.
Discussion
Less
Recently, numerous articles have shown that tumor infiltrating neutrophils are educated in the TME. Importantly, educated neutrophils maintain a cancer-promoting phenotype, which exhibit longer lifespan and release more protumorigenic substances such as MMP-9 and vascular endothelial growth factor to fuel tumor progression [8,10]. Others reported that tumor reprograms neutrophil through lipid accumulation in infiltrated neutrophils [9]. However, little is known about the resource of the lipids accumulated in neutrophils. This study reveals that lung cancer cells transported fatty acids to neutrophils via fatty acid-rich exosomes and enhanced FAO activity and promoted NETs formation to exacerbate lung cancer growth. Additionally, Rab34 was identified as a key regulator for exosome uptake in neutrophils (Fig. 7E).
Within the TME, a dynamic crosstalk occurs between immune cells and tumor cells, mediated by cytokines and other factors, which shapes their mutual behavior [19–21]. We and others have reported that lung cancer-educated neutrophils released NETs to promote tumor growth and metastasis in lung cancer tissues [6,10,33]. However, it is not clear which factor released by lung cancer cells is the key factors to activate neutrophils, thus inducing NETs formation. RNA-seq revealed that lung cancer-educated neutrophils significantly up-regulate lipid metabolism-related genes—a finding validated by enhanced neutral lipid staining (Nile Red/BODIPY 493/503) in tumor-infiltrating neutrophils. We further demonstrated that LDEs alone were sufficient to increase neutral lipid content in neutrophils to a level comparable to full tumor-CM. However, this effect was not observed with exosome-free lung cancer cell-CM. To identify the specific lipids responsible for inducing lipid accumulation and NET formation in neutrophils, we performed HPLC-MS/MS-based lipidomic profiling. The analysis revealed a marked increase in FFA levels in exosome-stimulated neutrophils. The BODIPYTM FL C16 fatty acid trafficking assay showed that lung cancer cells could transport fatty acids to neutrophils by exosomes directly. Additionally, cancer cell-derived exosomes enriched FFAs compared with lung epithelial noncancerous cells. High level of lipids in lung cancer cell-derived exosomes induced lipid accumulation in neutrophils, resulting in NETs formation, when compared with exosomes from noncancerous cells.
FFAs accumulation has been demonstrated to induce hyperactivation of tumor-infiltrating neutrophils [9]. In this process, we found that fatty acid enhanced the CPT1a-promoting FAO pathway, facilitating mtROS production and consequently promoting NETs formation. The protumor effect of exosome-primed neutrophils was abolished by DNase I-mediated NET depletion in vivo, demonstrating that NETs formation is critically involved in neutrophil-mediated tumor promotion. Previous reports found that tumor cells can secret several soluble cytokines to induce NETs formation directly, like interleukin-8, high-mobility group box 1, and granulocyte colony-stimulating factor in vivo and in vitro [34–36]. However, our work showed that exosome-free tumor cell-CM might contain soluble protein above and does not influence lipid levels in neutrophils, further indicating that the cytokines of tumor cell secretion induce NETs formation without promoting synthesis of FFAs and catabolism. Importantly, these also proved that neutrophils educated by tumor cells deliver lipids through exosomes without affecting lipid synthesis. At first glance, the coexistence of increased lipid accumulation and enhanced FAO may appear paradoxical. However, this is resolved by considering lipid flux: The massive influx of exogenous FFAs from LDEs exceeds oxidative capacity, resulting in net lipid accumulation despite FAO up-regulation. Our time-course data show that lipid accumulation precedes FAO activation, and etomoxir inhibits NETs but does not prevent initial lipid accumulation. Thus, FAO is a consequence of lipid overload, linking lipid accumulation to NETs formation. Our findings, integrated with existing evidence, reveal a sophisticated signaling network through which tumor cells educate neutrophils and instruct them to form NETs.
Excepting lipid metabolism changing in tumor-educated neutrophils showed by RNA-seq, the data strongly indicated that Rab34 was significantly up-regulated and negatively correlated with patient prognosis, which was confirmed at the protein expression level. It is well documented that the interaction between GTPase dynamin and Rab family proteins orchestrates key cellular processes, including internalization and the amplification of inflammatory signals [30–32]. Upon silencing GTPase proteins, we identified Rab34 as the primary regulator responsible for the internalization of lung cancer cell-derived exosomes and lung cancer progression induced by NETs. The established interplay between GTPase dynamin and the Rab family illustrates a complex regulatory network that governs cellular processes such as internalization. Silencing GTPase proteins highlights Rab34 as a crucial regulator and underscores its possible function in facilitating the internalization of lipid-rich exosomes within the TME. We further investigated whether Rab34 up-regulation is directly driven by exosomal FFAs. Our preliminary data showed that direct FFA supplementation alone was insufficient to induce Rab34 expression in neutrophils, suggesting that other exosomal components, such as proteins or nucleic acids, may be responsible for its transcriptional regulation. A comprehensive dissection of the upstream signals controlling Rab34 expression represents an important direction for future studies. This internalization process is crucial, as it can facilitate the transfer of mediators of lung cancer cells and promote tumor progression. Targeting Rab34 or its associated pathways may offer a strategic approach to mitigate inflammation and potentially enhance the efficacy of current cancer treatments. Therapeutically targeting this pathway holds translational potential for lung cancer by interrupting a critical communication axis that reprograms neutrophils toward a protumor phenotype.
The translation of these findings into clinical practice involves a multistage pathway. First, therapeutic agents that target Rab34 or specific NET components, such as peptidyl arginine deiminase 4 inhibitors, must be developed and tested for specificity and safety to avoid impairing beneficial immune functions. Second, their efficacy should be validated in advanced preclinical models, including patient-derived xenografts and orthotopic lung models, to confirm the mechanism within a human-relevant TME. Crucially, these novel agents ought to be evaluated in combination with standard therapies like immunotherapy, since NET disruption may help overcome treatment resistance. Concurrently, the development of biomarkers—such as NET signatures detected in liquid biopsies—is essential for identifying patients most likely to respond in future clinical trials, thereby enabling a targeted therapeutic strategy. This approach seeks to convert the protumoral neutrophil niche from a driver of progression into a therapeutic vulnerability.
While our study provides important insights into how LDEs reprogram neutrophils to promote tumor progression, several limitations should be considered. First, the translational potential of targeting Rab34 or NETs in clinical settings requires further validation using patient-derived samples or orthotopic models. Second, although lipidomics identified FFAs as key mediators, the study did not fully characterize the heterogeneity of exosomal lipids or rule out potential contributions from other cargo components. Third, while Rab34 knockdown attenuated exosome uptake and NETs formation, its broader roles in neutrophil function and potential off-target effects were not explored. Additionally, the direct causal relationship between exosomal FFAs, NETs, and clinical outcomes remains associative. Fourth, while our study establishes a critical role for Rab34 in neutrophil-mediated tumor progression, direct validation of Rab34 expression and its correlation with NETs markers in human lung cancer tissues remains to be addressed. Access to clinical samples and patient-derived neutrophils will be essential in future studies to strengthen the translational relevance of our findings. Future studies should measure NETs markers in patient samples to strengthen clinical relevance. Addressing these limitations will be crucial for developing targeted therapies against exosome-mediated neutrophil reprogramming in lung cancer.
Our findings elucidate a crucial tumor-neutrophil interaction, demonstrating the pivotal role of LDEs and the FAO pathway in driving NETs formation and tumor progression. Additionally, the identification of Rab34 as a key regulator of lung cancer cell-derived exosomes uptake and NETs formation suggests that Rab34 may serve as a potential therapeutic target for lung cancer treatment. This study provides a comprehensive understanding of the molecular mechanisms, underlying the interaction between lung cancer cells and neutrophils, and highlights the potential of targeting this interaction for the development of novel therapeutic strategies in the treatment of lung cancer.
Methods
Less
Study design
This study investigated the mechanism through which LDEs promote neutrophil reprogramming and tumor progression by inducing NETs formation, employing integrated in vitro and in vivo approaches. RNA-seq of neutrophils treated with lung cancer cell-CM identified altered signaling pathways. Lipidomic profiling via HPLC-MS/MS further characterized lipid accumulation in neutrophils. Functional assays—including exosome uptake, fatty acid transfer, and NETs formation—evaluated metabolic reprogramming and activation of neutrophils. Syngeneic mouse models, using C57BL/6J mice injected with LLC cells, assessed the roles of Rab34 and NETs in vivo. The sample sizes for all animal experiments (n = 4 to 5 per group) were justified by prior data to ensure 80% power at an alpha of 0.05, with mice randomized before the initiation of treatment. Exact values of n can be found in the figure legends. Herein, the term “n” connotes biologically independent samples: specifically, the number of individual animals for in vivo studies and the count of independent cultures or isolations for in vitro analyses. Moreover, every major finding was corroborated in a minimum of 3 separate experiments, and technical replicates were employed solely in instances that are clearly indicated.
Cell culture
The following cell lines were used: LLC (CL-0140; Procell), A549 (CL-0016; Procell), and HL-60 (CL-0110; Procell), cultured in Dulbecco’s modified Eagle’s medium, F12, and RPMI 1640 media (KeyGEN, China), respectively; Beas2B (FH0319; Fuheng) and MLE (FH1103; Fuheng) cells, both cultured in RPMI 1640. All cultures were maintained at 37 °C with 5% CO₂ in medium containing 10% fetal bovine serum (Sunrise, USA) and 1% penicillin–streptomycin (Beyotime, China).
Neutrophil collection
Human neutrophil-like cells were modeled by differentiating HL-60 cells into dHL-60 cells using an established protocol. In brief, cells were treated with 1.3% dimethyl sulfoxide in complete RPMI 1640 medium (supplemented with 10% fetal bovine serum) for 5 to 7 d to induce granulocytic differentiation. The mouse BMN isolation was carried out according to the protocol as described by our previously papers [10]. Tumor-infiltrated neutrophils were isolated by BD FACSAria III from tumor tissue single-cell suspension.
Lentiviral production
Pseudoviral particles for gene silencing were generated using control short hairpin (sh)RNA plasmids and shRNA plasmids specific for human Rab34, human and mouse FASN, human SMPD2, and human CPT1a, which were obtained from the MiaoLing Plasmid Platform (Wuhan, China). These plasmids were cotransfected with the helper plasmids pMD2.G and psPAX2 into 293T packaging cells. The viral supernatant was collected 48 h after transfection and used to transduce the corresponding cells for gene suppression. After transduction, the cells underwent puromycin selection for 3 d. Finally, western blot analysis confirmed the knockdown efficiency of the target proteins.
Isolation of LDEs
Lung cancer cell-CM was prepared as described. Exosomes were isolated via ultracentrifugation following an established protocol [37]. Briefly, the medium underwent serial centrifugation steps at 4 °C: 350 g and 2,000 g for 10 min each, followed by 12,000 g for 40 min, to remove cells and debris. The supernatant was then passed through a 0.2-μm filter (PN4612; Pall, Westborough, MA, USA) and subjected to ultracentrifugation (Beckman Coulter, Brea, CA, USA) at 120,000 g for 70 min (4 °C) to pellet the exosomes.
The condensed pellet was washed with ice-cold phosphate-buffered saline (PBS) and centrifuged again at 120,000 g for another 70 min at 4 °C. The resulting pelleted exosomes were suspended in PBS, and concentrations of exosome proteins were measured using the BCA Protein Assay Kit (Beyotime, Shanghai, China).
Isolated exosomes were analyzed for particle size and zeta potential on a Malvern ZetaSizer Nano system. Furthermore, western blotting was performed to confirm the presence of the exosomal marker CD9 and the absence of the endoplasmic reticulum protein calnexin, serving as a negative control. The morphology of the exosomes was observed using a biological electron microscope.
GFP-positive exosomes preparation
To produce CD9-GFP pseudoviruses, 293T cells were cotransfected with the pLV3-CMV-CD9-EGFP-Puro plasmid (Miaoling Biology, China) and the packaging plasmids pMD2.G and psPAX2. The supernatant containing the viral particles was harvested after 48 h and employed to infect LLC cells. Transfection efficiency was analyzed by flow cytometry after 3 consecutive days of puromycin screening. Exosomes from CD9-GFP-positive were isolated as above, and GFP intensity of exosomes was confirmed by a Cytation 3 Cell Imaging MultiMode Reader.
RNA-seq for tumor-educated neutrophils
CM was collected from LLC and A549 cells after 48-h culture in serum-free Dulbecco’s modified Eagle’s medium and F12 medium, respectively. Cell-free medium, processed identically in the absence of cells, served as the control. Neutrophils were then stimulated with or without CM for 4 h at 37 °C, after which cell pellets were harvested. Total RNA was extracted using TRIzol reagent (Invitrogen). RNA-seq was performed by CapitalBio Technology (Beijing), and the resulting raw reads were quality-controlled with FastQC, adapter-trimmed, and aligned to the reference genome using HISAT2. Gene expression was quantified by featureCounts, and differentially expressed genes were identified with DESeq2 (∣log₂FC∣ > 1, adjusted P < 0.05). Functional enrichment of differentially expressed genes was analyzed via Reactome and Kyoto Encyclopedia of Genes and Genomes pathway databases.
Nile Red staining
Neutrophils were treated with lung cancer cell-CM or 40 μg/ml exosomes for 0 to 4 h at 37 °C. Cells were then stained with 0.5 μM Nile Red for 10 min at room temperature, followed by 3 washes with PBS. Fluorescence intensity was measured using either a Cytation 3 Cell Imaging Multi-Mode Reader (BioTek; excitation/emission: 559/635 nm) or a BD FACSCanto II flow cytometer.
Mitochondrial mass
Neutrophils (1 × 107/ml) were incubated with 40 μg/ml exosomes for 4 h at 37 °C. After being washed 3 times with PBS, the cells were stained with 70 nM MitoTracker for 10 min at room temperature and washed again. Fluorescence intensity was then measured using a Cytation 3 Cell Imaging Multi-Mode Reader (BioTek, Winooski, VT).
Mitochondrial ROS
Neutrophils (1 × 107/ml) were treated with 40 μg/ml exosomes for 4 h at 37 °C. After washing 3 times with PBS, the cells were incubated with 1 μM MitoSOX for 10 min at room temperature. Following another wash cycle, fluorescence intensity was measured using a Cytation 3 Cell Imaging Multi-Mode Reader (BioTek).
Confocal microscopy
Neutrophils were first incubated with lung cancer cell-CM for 4 h at 37 °C. The cells were then allowed to adhere onto poly-L-lysine-coated glass coverslips in culture plates. After fixation, the adherent neutrophils were stained with BODIPY 493/503 (for neutral lipids) and Hoechst (for nuclei) and finally imaged using a Zeiss LSM880 confocal microscope (Oberkochen, Germany).
For exosome uptake, mouse BMNs were incubated with GFP-exosomes for 2 h and then allowed to adhere to glass coverslips for 30 min. Following fixation, the adherent neutrophils were stained with Dil to label the cell membrane and with Hoechst for 10 min. Images were acquired using a Zeiss LSM880 confocal microscope (Oberkochen, Germany).
Enzyme-linked immunosorbent assay
Following a 4-h stimulation with lung cancer cell-CM at 37 °C, neutrophil supernatants were collected by centrifugation (500 g, 5 min, 4 °C). MPO–DNA levels in the supernatant were measured using a specific enzyme-linked immunosorbent assay kit (Jiangsu Meimian) according to the manufacturer’s protocol.
To quantify intratumoral MPO–DNA concentrations, equal weights of tumor tissue were homogenized in an equivalent volume of PBS. The homogenate was centrifuged, and the supernatant was collected. MPO–DNA levels were then measured using enzyme-linked immunosorbent assay kits.
Fatty acid detection assay
After a 4-h incubation with LDEs at 37 °C, neutrophils were collected by centrifugation at 500 g for 5 min at 4 °C. The FFA content in both neutrophils and exosomes was then quantified using a commercial FFA assay kit (Enzyme-linked Biotechnology Co., Ltd, China), in accordance with the manufacturer’s instructions.
Fatty acid transfer assay
LLC or A549 cells were first labeled by culturing with BODIPY FL C16—a fluorescent fatty acid analog—for 24 h. After washing with PBS, the labeled cells were further incubated in serum-free RPMI 1640 medium for 48 h. The CM was collected, and exosomes were isolated via ultracentrifugation as previously described. Subsequently, BMNs or dHL-60 cells were incubated with these labeled exosomes for 4 h. Fluorescence intensity (Ex/Em: 505/512 nm) in tumor cells, exosomes, and neutrophils was measured using a Cytation 3 Cell Imaging Multi-Mode Reader.
Western blot
Isolated LDEs were lysed in sodium dodecyl sulfate-polyacrylamide gel electrophoresis loading buffer (P0015F, Beyotime) and denatured at 100 °C for 10 min. Proteins were separated on 12% sodium dodecyl sulfate-polyacrylamide gels and transferred to membranes. The membranes were probed with the following primary antibodies (1:1,000 dilution): anti-CitH3 (ab5103, Abcam), anti-Rab34, anti-CPT1a, anti-CD9, anti-CD63, and anti-actin (all from Cell Signaling Technology). Immunoreactive bands were visualized using an enhanced chemiluminescence chemiluminescent detection system (Thermo Scientific) and imaged with a Tanon imaging system. Band intensity was quantified using ImageJ software (National Institutes of Health).
Fatty acid mixture
The fatty acid mixture was prepared according to a published protocol [24]. Briefly, fatty acid stocks (200 mM) of palmitic (C16:0), stearic (C18:0) and oleic acid (C18:1) were prepared in 96% ethanol by heating at 70 °C with shaking, then equilibrated at 37 °C. Each stock was diluted 1:10 in prewarmed 10% FA-free bovine serum albumin (BSA) to a final concentration of 20 mM. The mixtures were vortexed (30 s) and incubated with gentle agitation at 55 °C (15 min) followed by 37 °C. The solutions were then filtered through a 0.2-μm membrane. Neutrophils were treated with each fatty acid at a final concentration of 100 μM for 4 h. Control cells received equivalent BSA and ethanol vehicle.
Quantitative real-time PCR assay
BMNs were incubated with LLC-EXOs (40 μg/ml, 4 h) and subjected to RNA extraction using TRIzol. After cDNA synthesis (HiScript RT-PCR Kit), quantitative PCR was carried out on an ABI PRISM 7500 system (95 °C for 10 min; 40 cycles of 95 °C/10 s and 60 °C/34 s). Gene expression of FAO/oxidative phosphorylation-related targets (e.g., cpt1a, cpt2, acadvl, and ndufs1) was analyzed with β-actin as reference (primers in Table S1).
cfDNA detection
The concentration of cfDNA in the supernatant was quantified using Sytox Green Nucleic Acid Staining (Invitrogen). Briefly, 200 μl of supernatant was mixed with 1 μM Sytox Green in a 96-well plate and incubated in the dark at room temperature for 20 min. Fluorescence intensity was then measured at an emission wavelength of 523 nm using a Cytation 3 Cell Imaging Multi-Mode Reader (BioTek).
Lipidomics analysis
For neutrophils lipidomics analysis, BMNs (1 × 107/ml) were stimulated by LLC-exosomes (40 μg/ml) for 4 h at 37 °C. The neutrophil suspension was centrifuged, and the neutrophils were collected and quantified by HPLC-MS/MS analysis as described previously [38]. All identified lipid species were verified using authentic standards. Metabolite abundances were normalized to neutrophil counts, and integrated peak areas (reflecting metabolite concentrations) were quantified with MetaboAnalyst 3.0 [39].
Seahorse extracellular flux analysis
To measure fatty acid oxidation, BMNs were seeded at 200,000 cells per well in Seahorse XF96 plates with or without exosomes (40 μg/ml) and centrifuged at 400 g for 5 min to settle the cells. After 4 h, OCRs were determined using a Seahorse XFe96 analyzer (Agilent, CA, USA) according to the manufacturer’s protocol. One hour before the assay, the medium was replaced with FAO assay medium, consisting of Krebs–Henseleit buffer supplemented with 2.5 mM glucose, 0.5 mM carnitine, and 5 mM Hepes (pH 7.4). Palmitate was added to a final concentration of 0.1 mM immediately prior to measurement. The following compounds were injected sequentially during the OCR run at these final concentrations: 40 μM etomoxir, 1.5 μM oligomycin, 1 μM carbonyl cyanide p-trifluoromethoxyphenylhydrazone, and 0.5 μM each of rotenone and antimycin A.
Evaluation of cell viability
Neutrophils (BMNs or dHL-60) were treated with or without LDEs (40 μg/ml) for 4 h and in the presence or absence of DNase I (100 U/ml). The CM was subsequently collected, centrifuged to remove debris, and transferred to LLC or A549 cells in 96-well plates. Following incubation for 24, 48, or 72 h, we assessed cell viability using the Cell Counting Kit-8 assay according to the manufacturer’s instructions. Absorbance was measured at 450 nm using a microplate reader.
Preparation of Rab34-siRNA liposomes
Liposomes were prepared as previously described [38] by combining L-α-phosphatidylcholine, cholesterol, PEG2000-DSPE, and siRNA (Rab34 or control) at a molar ratio of 70:30:2:2.8 in chloroform. The solvent was evaporated using a rotary vacuum evaporator, and the resulting lipid film was hydrated with 250 mM ammonium sulfate via water bath sonication for 5 min. The liposomes were then resuspended in PBS (137 mM NaCl, 2.7 mM KCl, 8 mM Na₂HPO₄, and 2 mM KH₂PO₄, pH 7.4) to form micellar colloids. The Rab34-siRNA sequences used are provided in Table S2.
Mouse models
Wild-type male C57BL/6J mice (6 to 8 weeks old) were sourced from Xuzhou Medical University Animal Center and maintained under standard conditions. All animal experiments were performed in compliance with the university’s ethical guidelines following approval by the Institutional Animal Ethics Committee.
For neutrophils and LDEs coinjection mouse model, mice were inoculated with 3 × 105/100 μl of LLC cells subcutaneously according to our previously report [10]. When tumor volume reached to 50 mm3, 5 × 105 neutrophils or neutrophils precultured with 40 μg/ml LDEs for 2 h were injected on the paratumor side every 3 d for 3 times. Tumor growth was monitored every other day.
For NETs depletion in vivo, mouse lung cancer model was established as above. DNase I (5 mg/kg) was injected intraperitoneally every day after tumor volume reaching to 50 mm3. Tumor growth was monitored every other day.
For Rab34 knockdown in neutrophils, mouse lung cancer model was established as above. BMNs were cultured with Rab34-siRNA liposomes for 4 h and injected into the paratumor side after washing with PBS every 3 d for 3 times. Mice were monitored every other day for tumor development. Upon completion of the 20-d treatment period, the animals were euthanized and the tumors were collected for analysis.
To establish the orthotopic lung cancer model, 8 × 105 LLC cells suspended in 50 μl of Matrigel were implanted into the left lung of each mouse. One week postimplantation, the subjects were allocated into 3 distinct experimental groups: a PBS control, a group receiving BMNs treated with control siRNA and LLC-derived exosomes (BMNs-Ctrl-siRNA+EXOs), and a group receiving BMNs treated with Rab34 siRNA and LLC-derived exosomes (BMNs-Rab34-siRNA+EXOs). These interventions were administered via retro-orbital injection every 3 d for a total of 3 doses. Throughout the study, body weights were recorded. After 20 d, all animals were humanely euthanized, and the tumor tissues were harvested for subsequent analysis.
Isolation of tumor-infiltrating immune cells
Tumor tissues were harvested, minced, and mechanically dissociated. The single-cell suspensions were filtered through a 40-μm cell strainer. Cells were stained with fluorochrome-conjugated antibodies specific for CD45, CD11b, Ly6G, and F4/80 (Biolegend). Using a BD FACSAria III flow cytometer, we sorted tumor-infiltrating neutrophils (CD45+/CD11b+/Ly6G+) and macrophages (CD45+/CD11b+/F4/80+). The sorted populations were collected directly into RIPA lysis buffer for protein extraction, and Rab34 expression was subsequently assessed by western blot.
Immunofluorescent staining
Tumor tissues were fixed in 4% PFA, OCT-embedded, and cryo-sectioned (5 μm). After permeabilization (0.1% Triton X-100) and blocking (10% BSA), sections were stained with anti-CitH3/MPO antibodies overnight, followed by Alexa Fluor-conjugated secondary antibodies. Images were acquired on Leica DM4000B and TCS SP8 systems.
Statistical analysis
Unless otherwise specified, data are presented as means ± standard error of the mean (SEM). Statistical significance was determined using GraphPad Prism 8.0, with unpaired t tests for 2-group comparisons and 1-way ANOVA (Tukey’s test) for multiple groups. A P value < 0.05 was deemed significant.
References
Less
1.
Bray F, Laversanne M, Sung H, Ferlay J, Siegel RL, Soerjomataram I, Jemal A.Global cancer statistics 2022: GLOBOCAN estimates of incidence and mortality worldwide for 36 cancers in 185 countries. CA Cancer J Clin. 2024;74(3):229–263.
2.
Altorki NK, Markowitz GJ, Gao D, Port JL, Saxena A, Stiles B, McGraw T, Mittal V.The lung microenvironment: An important regulator of tumour growth and metastasis. Nat Rev Cancer. 2019;19(1):9–31.
3.
Kargl J, Busch SE, Yang GH, Kim KH, Hanke ML, Metz HE, Hubbard JJ, Lee SM, Madtes DK, McIntosh MW, et al.Neutrophils dominate the immune cell composition in non-small cell lung cancer. Nat Commun. 2017;8:14381.
4.
Yu L, Liebenberg K, Shen Y, Liu F, Xu Z, Hao X, Wu L, Zhang W, Chan HL, Wei B, et al.Tumor-derived arachidonic acid reprograms neutrophils to promote immune suppression and therapy resistance in triple-negative breast cancer. Immunity. 2025;58(4):909–925 e907.
5.
Cheng Y, Mo F, Li Q, Han X, Shi H, Chen S, Wei Y, Wei X.Targeting CXCR2 inhibits the progression of lung cancer and promotes therapeutic effect of cisplatin. Mol Cancer. 2021;20(1):62.
6.
He XY, Gao Y, Ng D, Michalopoulou E, George S, Adrover JM, Sun L, Albrengues J, Daßler-Plenker J, Han X, et al.Chronic stress increases metastasis via neutrophil-mediated changes to the microenvironment. Cancer Cell. 2024;42(3):474–486 e412.
7.
Wang D, Li X, Jiao D, Cai Y, Qian L, Shen Y, Lu Y, Zhou Y, Fu B, Sun R, et al.LCN2 secreted by tissue-infiltrating neutrophils induces the ferroptosis and wasting of adipose and muscle tissues in lung cancer cachexia. J Hematol Oncol. 2023;16(1):30.
8.
Ng MSF, Kwok I, Tan L, Shi C, Cerezo-Wallis D, Tan Y, Leong K, Calvo GF, Yang K, Zhang Y, et al.Deterministic reprogramming of neutrophils within tumors. Science. 2024;383(6679):Article eadf6493.
9.
Veglia F, Tyurin VA, Blasi M, de Leo A, Kossenkov AV, Donthireddy L, To TKJ, Schug Z, Basu S, Wang F, et al.Fatty acid transport protein 2 reprograms neutrophils in cancer. Nature. 2019;569(7754):73–78.
10.
Han L, Chen Y, Huang N, Zhou X, Lv Y, Li H, Chai D, Zheng J, Wang G.Cancer-educated neutrophils promote lung cancer progression via PARP-1-ALOX5-mediated MMP-9 expression. Cancer Biol Med. 2024;21(2):175–192.
11.
Adrover JM, McDowell SAC, He XY, Quail DF, Egeblad M.NETworking with cancer: The bidirectional interplay between cancer and neutrophil extracellular traps. Cancer Cell. 2023;41(3):505–526.
12.
He D, Wu Q, Tian P, Liu Y, Jia Z, Li Z, Wang Y, Jin Y, Luo W, Li L, et al.Chemotherapy awakens dormant cancer cells in lung by inducing neutrophil extracellular traps. Cancer Cell. 2025;43(9):1622–1636.e27.
13.
Brinkmann V, Reichard U, Goosmann C, Fauler B, Uhlemann Y, Weiss DS, Weinrauch Y, Zychlinsky A.Neutrophil extracellular traps kill bacteria. Science. 2004;303(5663):1532–1535.
14.
Yang L, Liu Q, Zhang X, Liu X, Zhou B, Chen J, Huang D, Li J, Li H, Chen F, et al.DNA of neutrophil extracellular traps promotes cancer metastasis via CCDC25. Nature. 2020;583(7814):133–138.
15.
Xiao Y, Cong M, Li J, He D, Wu Q, Tian P, Wang Y, Yang S, Liang C, Liang Y, et al.Cathepsin C promotes breast cancer lung metastasis by modulating neutrophil infiltration and neutrophil extracellular trap formation. Cancer Cell. 2021;39(3):423–437.e27.
16.
Rayes RF, Mouhanna JG, Nicolau I, Bourdeau F, Giannias B, Rousseau S, Quail D, Walsh L, Sangwan V, Bertos N, et al.Primary tumors induce neutrophil extracellular traps with targetable metastasis promoting effects. JCI. Insight. 2019;5(16).
17.
Ren J, He J, Zhang H, Xia Y, Hu Z, Loughran P, Billiar T, Huang H, Tsung A.Platelet TLR4-ERK5 axis facilitates NET-mediated capturing of circulating tumor cells and distant metastasis after surgical stress. Cancer Res. 2021;81(9):2373–2385.
18.
Mousset A, Lecorgne E, Bourget I, Lopez P, Jenovai K, Cherfils-Vicini J, Dominici C, Rios G, Girard-Riboulleau C, Liu B, et al.Neutrophil extracellular traps formed during chemotherapy confer treatment resistance via TGF-beta activation. Cancer Cell. 2023;41(4):757–775.e10.
19.
McAllister SS, Weinberg RA.The tumour-induced systemic environment as a critical regulator of cancer progression and metastasis. Nat Cell Biol. 2014;16(8):717–727.
20.
Lucotti S, Kenific CM, Zhang H, Lyden D.Extracellular vesicles and particles impact the systemic landscape of cancer. EMBO J. 2022;41(18):Article e109288.
21.
Liu C, Chen Y, Xu X, Yin M, Zhang H, Su W.Utilizing macrophages missile for sulfate-based nanomedicine delivery in lung cancer therapy. Research. 2024;7:0448.
22.
Buzas EI.The roles of extracellular vesicles in the immune system. Nat Rev Immunol. 2023;23(4):236–250.
23.
Lim AR, Rathmell WK, Rathmell JC.The tumor microenvironment as a metabolic barrier to effector T cells and immunotherapy. eLife. 2020;9:Article e55185.
24.
Yin X, Zeng W, Wu B, Wang L, Wang Z, Tian H, Wang L, Jiang Y, Clay R, Wei X, et al.PPARalpha inhibition overcomes tumor-derived exosomal lipid-induced dendritic cell dysfunction. Cell Rep. 2020;33(3):Article 108278.
25.
Chen Y, Han L, Qiu X, Wang M, Chen Z, Cai Y, Xin Y, Lv Y, Hu A, Chai D, et al.Reassembling of albumin-bound paclitaxel mitigates myelosuppression and improves its antitumoral efficacy via neutrophil-mediated targeting drug delivery. Drug Deliv. 2022;29(1):728–742.
26.
Chen Y, Zhao C, Guo H, Zou W, Zhang Z, Wei D, Lu H, Zhang L, Zhao Y.Wip1 inhibits neutrophil extracellular traps to promote abscess formation in mice by directly dephosphorylating Coronin-1a. Cell Mol Immunol. 2023;20(8):941–954.
27.
Hu S, Zhang F, Wang J, Zhang J, Li C, Lyu Y, Wang Y, Huang R, Gao Y, Yang H, et al.MMP9(high) neutrophils are critical mediators of neutrophil extracellular traps formation and myocardial ischemia/reperfusion injury. Adv Sci. 2025;12(21):Article e2415205.
28.
Kelly DP, Scarpulla RC.Transcriptional regulatory circuits controlling mitochondrial biogenesis and function. Genes Dev. 2004;18(4):357–368.
29.
Wang Y, Chen T, Han C, He D, Liu H, An H, Cai Z, Cao X.Lysosome-associated small Rab GTPase Rab7b negatively regulates TLR4 signaling in macrophages by promoting lysosomal degradation of TLR4. Blood. 2007;110(3):962–971.
30.
Lian H, Jiang K, Tong M, Chen Z, Liu X, Galán JE, Gao X.The Salmonella effector protein SopD targets Rab8 to positively and negatively modulate the inflammatory response. Nat Microbiol. 2021;6(5):658–671.
31.
Ganga AK, Kennedy MC, Oguchi ME, Gray S, Oliver KE, Knight TA, de la Cruz EM, Homma Y, Fukuda M, Breslow DK.Rab34 GTPase mediates ciliary membrane formation in the intracellular ciliogenesis pathway. Curr Biol. 2021;31(13):2895–2905 e2897.
32.
Ye H, Yang Q, Guo H, Wang X, Cheng L, Han B, Hong M, Ma F, Li M, Wu X, et al.Internalisation of neutrophils extracellular traps by macrophages aggravate rheumatoid arthritis via Rab5a. RMD Open. 2024;10(1):Article e003847.
33.
Wang Y, Liu F, Chen L, Fang C, Li S, Yuan S, Qian X, Yin Y, Yu B, Fu B, et al.Neutrophil extracellular traps (NETs) promote non-small cell lung cancer metastasis by suppressing lncRNA MIR503HG to activate the NF-kappaB/NLRP3 inflammasome pathway. Front Immunol. 2022;13:Article 867516.
34.
Yang L, Liu L, Zhang R, Hong J, Wang Y, Wang J, Zuo J, Zhang J, Chen J, Hao H.IL-8 mediates a positive loop connecting increased neutrophil extracellular traps (NETs) and colorectal cancer liver metastasis. J Cancer. 2020;11(15):4384–4396.
35.
Zhang X, Shi H, Yuan X, Jiang P, Qian H, Xu W.Tumor-derived exosomes induce N2 polarization of neutrophils to promote gastric cancer cell migration. Mol Cancer. 2018;17(1):146.
36.
Bun M, Kawano M, Yamamoto G, Sakata M, Shimura K, Toda A, Nakamura K, Kinose Y, Kodama M, Hashimoto K, et al.G-CSF induces neutrophil extracellular traps formation and promotes ovarian cancer peritoneal dissemination. J Leukoc Biol. 2024;116(5):1157–1168.
37.
Yang J, Dang G, Lü S, Liu H, Ma X, Han L, Deng J, Miao Y, Li X, Shao F, et al.T-cell-derived extracellular vesicles regulate B-cell IgG production via pyruvate kinase muscle isozyme 2. FASEB J. 2019;33(11):12780–12799.
38.
Han L, Miao Y, Zhao Y, Zhang X, Ma X, du X, Kong W, Xu Q, Liu J, Dai K, et al.The binding of autotaxin to integrins mediates hyperhomocysteinemia-potentiated platelet activation and thrombosis in mice and humans. Blood Adv. 2022;6(1):46–61.
39.
Xia J, Sinelnikov IV, Han B, Wishart DS.MetaboAnalyst 3.0—making metabolomics more meaningful. Nucleic Acids Res. 2015;43(W1):W251–W257.
Appendix
Less
Year 2026 volume 9 Issue 5
PDF
79
43
Cite this Article
BibTeX
Article Info
doi: 10.34133/research.1278
  • Receive Date：2025-11-10
  • Online Date：2026-10-16
  • Published：2026-05-20
Article Data
Affiliations
History
  • Received：2025-11-10
  • Revised：2026-03-23
  • Accepted：2026-04-13
Affiliations
    1Cancer Institute, Xuzhou Medical University, 209 Tongshan Road, Xuzhou 221004, China.
    2Center of Clinical Oncology, The Affiliated Hospital of Xuzhou Medical University, 99 West Huaihai Road, Xuzhou 221002, China.
    3Jiangsu Center for the Collaboration and Innovation of Cancer Biotherapy, Xuzhou Medical University, 209 Tongshan Road, Xuzhou 221004, China.

Corresponding:

* Address correspondence to: (L.H.);
* Address correspondence to: (L.L.);
* Address correspondence to: (G.W.)
References
Share
https://castjournals.cast.org.cn/joweb/research/EN/10.34133/research.1278
Share to
QR

Scan QR to access full text

Cite this article
BibTeX
Citations
表12种不同金属材料的力学参数
科
Family		 属数
Number of
genus		 种数
Number of
species		 占总种数比例
Percentage of
total species (%)		 属
Genus		 种数
Number of
species		 占总种数比例
Percentage of total
species (%)
鹅膏菌科Amanitaceae 2 11 5.26 鹅膏菌属 Amanita 10 4.78
小菇科 Mycenaceae 2 12 5.74 丝盖伞属 Inocybe 5 2.39
多孔菌科 Polyporaceae 8 14 6.70 蜡蘑属 Laccaria 5 2.39
红菇科 Russulaceae 3 23 11.00 小皮伞属 Marasmius 6 2.87
小菇属 Mycena 11 5.26
光柄菇属 Pluteus 5 2.39
红菇属 Russula 17 8.13
栓菌属 Trametes 5 2.39
关闭全屏
  • BibTeX
  • EndNote
  • RefWorks
  • TxT
Links
Articles
Latest Articles
Most Read
Collections
Updates
Events
News
Multimedia
About
About Us
Contact
No. 86 Xueyuan South Road, Haidian District, Beijing
100081
010-62662699(Operation and Technical Support)
qkjq@cast.org.cn

Copyright © 2025 China Association for Science and Technology. All rights reserved. For all open access content, the relevant licensing terms apply.
Sponsored by the Office of the Leading Group for Cybersecurity and Informatization of CAST, and supported by Science and Technology Review Publishing House