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Therapeutic options for premature ovarian insufficiency: an updated review


Primary ovarian insufficiency (POI) is a rare gynecological condition. This disease causes menstrual disturbances, infertility, and various health problems. Historically, hormone replacement therapy is the first-line treatment for this disorder. Women diagnosed with POI are left with limited therapeutic options. In order to remedy this situation, a new generation of therapeutic approaches, such as in vitro activation, mitochondrial activation technique, stem cell and exosomes therapy, biomaterials strategies, and platelet-rich plasma intra-ovarian infusion, is being developed. However, these emerging therapies are yet in the experimental stage and require precise design components to accelerate their conversion into clinical treatments. Thus, each medical practitioner bears responsibility for selecting suitable therapies for individual patients. In this article, we provide a timely analysis of the therapeutic strategies that are available for POI patients and discuss the prospects of POI therapy.


Primary ovarian insufficiency (POI), also referred to as premature ovarian failure (POF), pertains to the loss of ovarian function under the age of 40 years [1]. It is characterized by a decrease in ovarian follicles, and a dirth of hormone secretion. Although the prevalence of POI was previously reported as varying between 0.9–1.2% [2], a national register study conducted in Sweden has indicated that the total prevalence of POI approximates 1.9% [3]. A recent meta-analysis conducted by Golezar et al., estimated that 3.7% of women worldwide are affected [4]. POI patients experience long term complications, such as osteoporosis, fractures, cardiovascular diseases and depression [5]. Furthermore, this disease shows great potential for destroying the hopes and dreams of parenthood.

Diagnostic criteria for POI include oligo/amenorrhea for at least 4 months and two elevated follicle-stimulating hormone (FSH) levels (> 25 IU/L) more than 4 weeks apart [6]. A delay in diagnosing POI may cause irreversible impairment to the fertility of patients. Anti-Mullerian hormone (AMH) and antral follicle count (AFC) are other sensitive indicators are used to assess ovarian reserves.

POI is a heterogeneous disorder caused by genetic factors, autoimmune diseases, mitochondrial abnormalities, iatrogenic factors (including chemotherapy, radiotherapy, and surgical procedures), and environmental factors [7]. Additionally, a significant proportion of POI patients are idiopathic with undetermined etiology [8].

POI may be treated in one of several ways (Fig. 1). Hormone replacement therapy (HRT) should be regarded as a physiological replacement of estrogens (+ progestin), but it fails to restore ovarian function. Currently used novel strategies mainly include in vitro activation (IVA), mitochondrial activation, stem cell and exosomes therapy, biomaterials strategies and intra-ovarian infusion of platelet-rich plasma (PRP). However, these new therapies, which are expected to be breakthrough therapies for POI, are still in their experimental stages, and their efficacy and safety must be proven prior to acceptance as true clinical options. This review summarizes current and future therapeutic strategies for POI.

Fig. 1
figure 1

Several treatments of premature ovarian failure. For POI patients, HRT is the first-line treatment. In vitro activation, mitochondrial activation technique, stem cell and exosomes therapy, biomaterials strategies, and platelet-rich plasma intra-ovarian infusion are a new generation of treatments for POI management

Innovative therapeutic options for POI

In vitro activation

A previous study has indicated that approximately 75% of POI patients may carry residual dormant primordial follicles (PFs) in the ovaries [5]. The stored PFs of such patients may be effectively used to treat their infertility. Furthermore, IVA is a novel technique that stimulates the growth of PFs and induces these to develop into competent oocytes. In this manner, POI patients are able to produce offspring using their own genes.

Molecular regulation of IVA

IVA mainly involves phosphatase and tensin homolog (PTEN)/phosphatidylinositol-3-kinase (PI3K)/protein kinase B (Akt)/forkhead box O3 (FOXO3) signaling pathway, and the Hippo signaling pathways (Fig. 2). The PTEN/PI3K/Akt/FOXO3 pathway plays a central role in PFs activation. The cognate tyrosine kinase receptor initiates Akt activation signaling by enhancing PI3K activity, which converts secondary messenger, phosphatidylinositol-4,5-bisphosphate (PIP2), into phosphatidylinositol-3,4,5-triphosphate (PIP3). Subsequently, PIP3 activates phosphatidylinositol-dependent kinase 1 (PDK1), resulting in Akt activation [9], a key kinase in this pathway. Once Akt is activated, FOXO3a is hyperphosphorylated and undergoes nuclear exportation, eventually triggering PFs activation. Furthermore, Akt phosphorylates tuberous sclerosis 2 (TSC2), which inactivates TSC1/TSC2 complex and induces mammalian target of rapamycin complex (mTORC1). Subsequently, mTORC1 and its substrates promote PFs survival [10]. However, these events are reversed by the effects of PTEN, which negatively regulates this pathway by transforming PIP3 back to PIP2 [11].

Fig. 2
figure 2

The PTEN/ PI3K / Akt / FOXO3 and Hippo signaling pathways regulates primordial follicles activation

The Hippo signaling pathway acts as a conservative regulator of organ size [12]. It consists of different negative growth regulators that inactivate Yes-associated protein (YAP)/transcriptional co-activator PDZ-binding motif (TAZ) signaling through phosphorylation. YAP/TAZ signaling plays a significant role in promoting the expression of intercellular signal proteins. In the ovary, mechanical signals, as ovarian fragmentation, disrupt the Hippo pathway by increasing the polymerization of G-actin into F-actin, resulting in the nuclear translocation of YAP [13]. The transcriptional interaction between nuclear YAP and TAZ increases the expression of CCN growth factor and baculoviral IAP repeat-containing (BIRC), leading to PF growth [14].

PFs activation involves multiple factors. Bone morphogenetic proteins (BMPs) and growth and differentiation factor 9 (GDF-9) are known to participate in early folliculogenesis. A study has indicated that BMP4 promotes the transformation of primordial follicles to primary follicles in a mouse ovary culture [15]. GDF-9 and BMP15 reportedly protect granulose cells (GCs) from apoptosis and improve the survival rate of follicles [16]. Moreover, activins can promote oocyte survival and PFs formation via the Smad2/Smad3 pathway [17]. By contrast, AMH is considered as an inhibitor of PFs activation. In AMH-cultured rat ovaries, PFs remained static despite the presence of other stimuli [18].

Preclinical studies of IVA

IVA is based on a large number of animal experiments. For example, Adhikari et al. [19] treated mouse ovaries with PTEN inhibitor bpV for 24 h and then transplanted them into the kidney capsules of the matched ovary to generate mature oocytes. The study also confirmed that transient treatment with PTEN inhibitors did not cause tumor formation or other chronic illnesses in recipient mice. Additionally, the number of antral follicles was increased in ovaries co-treated with MHY1485 (an mTOR activator) and Akt stimulators [10]. Recently, Zhang et al. revealed that topical injection of epidermal growth factor and bio-gel into ovaries could activate PFs by elevating CDC42-PI3K signaling and the PI3K/Akt pathway in murine as well as human ovarian tissues [20].

These studies indicated that PTEN/PI3Kb signaling regulation can be applied to reproductive practice. However, the impact of this technology on the survival and function of follicles has raised concerns. PTEN inhibition promotes PFs activation, and is accompanied by DNA damage and impaired DNA repair competence [21]. This result may be explained away as being due to the high metabolic activity and proliferation rate of GCs following Akt activation [22]. Another explanation pertains to impaired contact between somatic cells and oocytes [23].

Although fragmentation of ovaries disrupts the Hippo pathway, existing animal studies have indicated that differences may exist in the degree of ovarian fragmentation [24]. Furthermore, the connection between actin polymerization and the Hippo signaling pathway offers another potential target for IVA. Studies have reported that incubating ovaries with drugs that promote actin polymerization, such as jasplakinolide or sphingosine-1-phosphate, induces actin polymerization accompanied by an increase in nuclear YAP, leading to follicle growth [25].

In recent years, the role played by mechanical stress in the interaction between ovarian cells and the microenvironment has attracted much attention. Although the collagen-rich ovarian cortex provides a rigid physical environment that supports the follicle structure, ovarian extracellular matrix (ECM) rigidity limits the development and maturation of the follicle [26]. Furthermore, ECM digestion may induce the nuclear export of FOXO3a and oocyte growth [27]. Deposition and remodeling of mechanical matrix components, such as collagen, elastin, elastin microfibril interface localization protein-1, and fibrin-1, are associated with early follicle activation [28]. The above findings indicate therapeutic targets at the ECM level.

Translation of IVA in the practice of human reproduction

IVA has been successfully applied in clinical practice. Conventional IVA in POI patients was the combination of PTEN inhibitors and PI3K activators, followed by ovarian fragmentation and autografting cortical strips via laparoscopic surgery. This procedure resulted in two pregnancies and one healthy delivery [14]. In 2016, Zhai et al. reported a successful delivery after simplifying IVA by fresh tissue auto-transplantation [29].

Drug-free IVA was developed more recently. It focuses only on disrupting the Hippo pathway and avoids chemical activation of ovaries. A growing number of studies have reported that drug-free IVA had led to successful pregnancies [30, 31]. However, these results should be interpreted with caution because most of these studies, involved a limited number of patients and lacked controlled trials.

IVA provides a beneficial option for cancer patients because this technology increases the effectiveness of activating PFs via ovarian tissue freezing which maximizes the number of available oocytes [32]. After the primary disease is alleviated, the patients can transplant activated ovarian tissue based on their individual reproductive wishes. Notably, tumor cells may remain in the transplants of tumor patients, and thus the application of follicular separation technology and in vitro culture systems are utilized to minimize the risk of tumor enhancement. Finally, the necessity for IVA in fertility preservation has been questioned due to the spontaneous activation of PFs occurring in conventional fertility preservation [33]. In addition, another study has reported that excessive activation of follicles cause follicle loss and shortens the lifespan of graft [34].

Mitochondrial activation technique

Mitochondria are the power sources of cells and the only organelles that contain a unique genome, termed mitochondrial DNA (mtDNA). Reportedly, mtDNA is a double-stranded, circular DNA with a length of approximately 16.5 kb, containing 37 genes encoding 13 protein, 2rRNAs, and 22 tRNAs [35]. The main function of mitochondria is to produce adenosine triphosphate (ATP) by oxidative phosphorylation [35]. In addition, mitochondria regulate other pathways, including calcium signaling, intracellular redox potential and apoptosis [36]. Mitochondria are also the primary source of intracellular reactive oxygen species (ROS). More importantly, the mitochondrial are tightly linked to oocytes quality and embryonic development.

Mitochondria and ovarian aging

Ovarian aging caused by mitochondrial dysfunction involves mtDNA dysfunction, enhanced oxidative damage, altered membrane potential and inefficient biogenesis or mitochondria clearance [37]. Of these, mtDNA dysfunction includes decreased mtDNA content, strand breaks, point mutations, and oxidative damage. Patients with POI reportedly exhibited significantly decreased mtDNA content compared to healthy fertile women [38]. Furthermore, mtDNA is prone to mutations due to the absence of histone protection and DNA repair enzymes [39]. Studies have shown that a single-point alteration in mtDNA profoundly influences mitochondrial proteostasis and reactive ROS generation, leading to telomere shortening [40]. Moreover, the introduction of mutated mtDNA polymerase gamma (POLG) into a mouse caused premature senescence [41].

ROS levels in POI populations are significantly higher [42]. Excessive accumulation of ROS drives mtDNA mutations and energy deficiency, consequently inducing aging [43]. In turn, mtDNA mutations further exacerbate the production of ROS. This vicious circle of self-amplification and destruction may lead to cell apoptosis. Additionally, overproduction of ROS may overwhelm cellular antioxidant defenses, leading to oxidative stress (OS) and premature aging [44].

Disturbances of mitochondrial dynamics, such as mitochondrial fusion, changes in mitochondrial metabolism, and imbalances in calcium homeostasis, also affect oocyte aging [43]. Mitofusin 2 (MFN2) is a key protein involved in mitochondrial fusion, causing oocytes lacking MFN2 that contributed to female infertility [45]. Mitochondrial fission factor dynamin-related protein 1(Drp1) is the key to maintaining oocyte quality. A previous study reported that Drp1 knockout may lead to follicular dysplasia and ovulation disorders [46]. Furthermore, the lack of mitochondrial proteases may lead to mitochondrial-related diseases and aggravate oocyte aging [47].

Mitochondrial nutrient therapy

In recent years, researchers have focused on using pharmacological methods to restore the vitality of mitochondria. Available mitochondrial nutrients include Coenzyme Q10 (CoQ10), resveratrol, melatonin, and rapamycin [48]. CoQ10 is a component of the mitochondrial electron transport chain and a cellular antioxidant, which reportedly delays the depletion of ovarian reserve [49]. Importantly, the only human trial conducted so far, has shown that supplementation with CoQ10 may reduce the rate of aneuploidy in oocytes after meiosis. However, the result of this study was not statistically significant due to the study being prematurely terminated due to safety considerations [50].

Resveratrol, an anti-aging compound, has been found to slow down ovarian aging and promote in vitro maturation of oocytes [48, 51]. However, resveratrol has not been recommended for routine clinical treatment due to an anti-deciduogenic effect that may reduce clinical pregnancy rate [52]. In addition, melatonin is considered to be an antioxidant against mitochondria. A published study showed that melatonin could delay ovarian aging in mice by increasing antioxidant capacity, maintaining telomerase activity and activating sirtuin1 [53].

Mitochondrial transfer therapy

Various mitochondrial transfer therapies have been tested for infertility management. A previous study has reported that allogeneic ooplasmic transfer in human oocytes led to successful pregnancy and live birth [54]. However, this technique was suspended due to the risk of heteroplasmy, and potential transmission of mitochondrial diseases, as well as Turner syndrome and autism cases being reported following transplantation [55]. Subsequently, new nuclear transplantation techniques, including spindle transplantation, germinal vesicle (GV) transplantation, and pronuclear transplantation (PNT), have been proposed.

Spindle transfer refers to the extraction of the spindle and its transplantation into an enucleated donor oocyte. In 2016, a study reported the first successful delivery by a woman with Leigh’s Syndrome (a rare mitochondrial disease) using this technique [56]. GV transfer, which improves meiotic resumption and oocyte maturation has been used against aneuploidy in infertile women [57]. However, it is noteworthy that mitochondria near the GV may be carried into reconstructed oocytes, leading to mitochondria heterogeneity, which adversely affecting offspring. Therefore, complete removal of mitochondria in patients is essential, although this remains a challenge in GV transfer. PNT involves the transfer of pronuclei from one zygote with abnormal mtDNA to another with healthy mtDNA. However, although PNT has led to triplet pregnancies [58], this technique is limited by ethical concerns due to the potential loss of zygotes.

Concerns regarding heteroplasmy resulted in the proposal of autonomous germline mitochondrial energy transfer (AUGMENT). The goal of AUGMENT is to isolate and obtain the mitochondria from oogonial stem cells and transfer them into the oocyte during intracytoplasmic sperm injection [59]. Oktay et al. revealed that women treated with AUGMENT showed high fertilization rates and embryonic scores. However, the authors failed to demonstrate a benefit for women > 40 years [60]. Furthermore, a well-designed random clinical trial questioned the effectiveness of AUGMENT, because women treated with AUGMENT showed lower mtDNA content and live birth rates than those in the control group [61]. Therefore, it may be concluded that current research on this procedure is preliminary at best, indicating that it is too early to apply AUGMENT to clinical practice.

Stem cell therapy

Stem cell therapy is expected to restore ovarian function and fertility for POI patients. Stem cells are early, undifferentiated cells with the ability to self-renew, unlimited proliferation, and multi-differentiation. They are classified as embryonic stem cells (ESCs), adult stem cells (ASCs), and induced pluripotent stem cells (iPSCs) according to their origin [62]. Mesenchymal stem cells (MSCs) are a subset of ASCs isolated from multiple tissues, including bone marrow, adipose tissue, menstrual blood, umbilical cord, amniotic fluid, and placenta [63].

Stem cell therapy mechanisms in POI

Stem cells exert their therapeutic effect by homing, differentiation and paracrine stimulation (Fig. 3). Stem cells that spontaneously migrate to the injured ovary are induced by multiple factors to adhere and proliferate. Current studies indicate that the therapeutic effect of stem cell transplantation may be mediated by paracrine mechanisms [64]. Paracrine signaling involves the secretion of multiple biologically active molecules, including growth factors, cytokines, regulatory factors, and signal peptides by surrounding cells to influence adjacent cells. This process improves the condition of damaged ovaries through anti-apoptosis, anti-fibrosis, angiogenesis, anti-inflammation, and immune regulation.

Fig. 3
figure 3

Stem cell therapy mechanisms in primary ovarian insufficiency. During ovarian insufficiency, stem cells play multiple roles through homing, differentiation and paracrine stimulation. Paracrine signaling is the key for the improvement of damaged ovaries through anti-apoptosis, anti-fibrotic, angiogenesis, anti-inflammation, and immune regulation. In addition,stem cell-mediated exosomes and mitochondrial transfer demonstrate another novel mechanism

Further investigation of paracrine signals indicates that stem cells secrete exosomes to mediate their functions. Exosomes are extracellular vesicles that carry proteins, mRNA, and microRNA (30-130 nm in size) [65]. These vesicles mediate cell-to-cell communication via target cell internalization, ligand-receptor interaction, or lipid membrane fusion [66]. Depending on their source cells, exosomes can initiate repair and regeneration processes to restore critical cellular functions and maintain tissue homeostasis thereby.

Stem cell-mediated mitochondrial transfer is another novel mechanism developed in recent years. Mitochondria are transferred from stem cells to adjacent cells through tunnel nanotubes, formed by pro-inflammatory cytokines that drive skeletal rearrangement in stem cells. It has also been recently reported that inflammation-driven transfer of mitochondria from stem cells to oocytes may rescue oocyte quality and embryo development [67, 68].

Stem cell therapy for POI

Although ESCs show unlimited potential for differentiation, clinical use of ESCs is limited. This is because the use of ESCs raises challenging ethical issues, such as the destruction of blastocysts. By contrast, iPSCs, which are prepared by reprogramming human somatic cells, may be used without any ethical issues. Yamashiro et al. confirmed that human iPSCs could differentiate into human primitive germ-like cells (hPGCLCs) in vitro. More importantly, hPGCLCs cultured under defined conditions differentiated into oogonia/gonocyte-like cells [69].

Significant progress has been made in the treatment of POI with MSCs (Table 1). Previous studies have reported that bone marrow stem cells (BMSCs) injected into mice reduced FSH levels and increased estrogen levels and follicle numbers, by increasing the secretion of vascular endothelial growth factor (VEGF) [70]. Furthermore, BMSCs could inhibit GC apoptosis by downregulating cyclin-dependent kinase inhibitor 1A (P21) and Bcl-2-associated X protein (Bax), and upregulating the c-myc proto-oncogene mRNA [71].

Table 1 Summary of stem cell therapy for POI

Adipose-derived stem cell (ADSCs), which are pluripotent and easy to access, are ideal therapeutic cells. A study demonstrated that ADSC implantation induces angiogenesis, restores the number of follicles and the corpus luteum, and repairs ovarian damage thereby [72]. Menstrual blood-derived mesenchymal stem cells (MenSCs) are increasingly attracting attention, due to the controversy regarding the non-ethical nature of their usage, as also low immune rejection and toxicity [100]. Previous studies have showed that MenSCs protected GCs from apoptosis and increased the secretion of fibroblast growth factor 2, thereby improving POI [73, 74].

In addition, placenta-derived mesenchymal stem cells (PMSCs) transplantation significantly increased serum AMH and estrogen, while dramatically reducing follicular atresia and GC apoptosis [75]. Based on the results of recent studies, the therapeutic mechanisms underlying the alleviation of POI by PMSCs may include: (i) restoration of ovarian function via the regulation of Th17/Tc17 and Th17/Treg cell ratios by the PI3K/Akt signaling pathway; (ii) upregulation of antioxidant factors, which has been shown to restore ovarian function in ovariectomized rats; and (iii) reduction of GC apoptosis by inhibiting the endoplasmic reticulum stress inositol-demanding enzyme 1signaling pathway [76,77,78].

Umbilical cord mesenchymal stem cells (UC-MSCs) are widely used to treat POI. Human UC-MSCs inhibited ovarian fibrosis in POI rats by regulating the differentiation of ovarian stromal cells via the transforming growth factor-β/Smad3 signaling pathway [79]. Additionally, human amniotic fluid stem cells (AFSCs) have shown potential for differentiating into primordial follicle oocytes in vitro [80]. Amnion mesenchymal stem cells (AMSCs) also reduced the expression of inflammatory cytokines, which inhibited ovarian inflammation in rats with POI. Pretreatment of AMSCs using low-intensity pulsed ultrasound, augmented anti-inflammatory effects [81].

Cell-free therapy for POI

Treating POI with exosomes is associated with higher clinical safety, because immune rejection and the risk of vascular obstruction and tumor mutation can be avoided by using exosomes. A recent study revealed that exosomal miR-644-5p derived from BMSCs targeted the regulation of p53 to suppress the apoptosis of GCs, thus alleviating POI [82]. In 2020, Yang et al. reported that BMSCs-derived exosomal miR-144-5p relieved POI by targeting PTEN to inhibit GC apoptosis [83]. In addition, overexpression of miR-21, a key miRNA that regulates apoptosis in BMSCs, repaired ovarian structure and function in rats, by downregulating PTEN and the programmed cell death protein 4 (PDCD 4) [84].

ADSC-derived exosomes restored ovarian function in POI patients by regulating the SMAD pathway [85]. Besides, exosomal miRNA-17-5p derived from UC-MSCs improved ovarian function by regulating SIRT7 [86]. Moreover, exosomal miR-10a and miR-146a derived from AFSCs were essential for inhibiting follicular atresia and increasing GC survival, wherein miR-10a plays a leading role [87]. Ding et al. reported that exosomal miR-320a, released from human AMSCs, delayed ROS production in POI by regulating Sirtuin4 [88].

Biomaterial strategies for POI

Stem cell transplantation leads to extreme cell loss. Consequently, biomaterials including collagen, alginate, and hyaluronic acid (HA) have to be introduced. Collagen is essential for maintaining biological activity. He et al. created collagen-rich, biomimetic 3D shells via microfluidic encapsulation, where follicle culture with these biomimetic capsules helped these to develop into the antral stage [92]. Su et al. used a collagen scaffold to enhance the retention of ADSCs in target organs [89]. Similarly, Ding et al. reported that UC-MSCs on collagen scaffolds activated follicles via the phosphorylation of FOXO3a and FOXO1 [90].

Alginates may be used for drug delivery due to their biocompatibility, non-immunogenicity, and hydrophilicity. These have been used for the culture of secondary and pre-antral follicles [93]. ADSCs co-encapsulated with ovarian follicles in an alginate-based 3D culture system supported follicle genesis, survival, and maturation in vitro, via the secretion of cytokines [91]. HA is another widely used biological material. Certain tissues, such as those of the uterus and ovaries, that have HA receptors are amenable to targeted therapy [94]. Importantly, HA levels in POI patients are relatively low, and thus HA supplementation can be effectively used to prevent chemically induced ovarian injury and improve ovarian function [95].

Safety and optimization measures for stem cell therapy

The safety of stem cells must be evaluated so that they can be standardized prior to clinical application. Tumorigenicity, immunogenicity, and heterogeneity of ESCs and iPSCs typically limit their application. Among these, tumorigenicity presents the most concerning issue. The factors associated with tumorigenesis are as follows: (i) residual undifferentiated and/or immature cells present in stem cell populations lead to incorrect patterning; (ii) reprogramming factors specific to induced iPSCs promote tumorigenesis; and (iii) genetic mutations induced by the expansion of stem cells in vitro may cause tumorigenicity [96]. Therefore, effective methods that ensure directional differentiation, strict procedures of purification, and careful selection of cell lines are of great significance in regard to the safety of this therapy.

With respect to immunogenicity, autologous stem cell transplantation is an ideal choice to eliminate rejection. However, allogeneic transplantation is preferred to autologous transplantation due to time and cost constraints. Although immunosuppressive agents are currently used to overcome allograft rejection, their side effects, such as higher infection risk, cannot be disregarded. The human leukocyte antigen (HLA), an important component of the human immune system, is critical for immune rejection. Therefore, researchers are attempting to circumvent immune rejection by matching HLA haplotypes or inactivating HLA genes. Furthermore, as no two cells are similar, researchers are focused on overcoming heterogeneity by converting stem cells to their naive and ground states. However, further research is needed to address these challenges.

Clinical trials conducted worldwide have indicated that MSCs with low immunogenicity and tumorigenicity are safe sources of stem cells [97]. However, the therapeutic effects of these cells are still affected by multiple factors, such as the quality and quantity of cell products amplified in vitro, route of injection, optimal dose, and timing of the treatment. To date, researchers and clinicians have not been able to address these issues effectively.

PRP intra-ovarian infusion

Mechanisms of PRP in POI

Intra-ovarian infusion of PRP is another novel approach to the treatment of POI. PRP is composed of high concentrations of platelets obtained from the peripheral blood of patients via centrifugation [98]. The efficiency of PRP depends mainly on their α-granule content, which is highly enriched in proteins, hormones, and growth factors [99]. The release of bioactive proteins promotes cell proliferation and differentiation [101]. In addition, activated platelets release high concentrations of hormones and growth factors, which stimulate angiogenesis as well as anabolism and inflammation control, thereby rapidly promoting the healing and regeneration of tissues [102]. Importantly, GDF-9, implicated in the maturation potential of oocytes, and mutated in POI, is also present in PRP [103].

The mechanisms underlying the role of PRP in the treatment of POI remain elusive. Several studies have reported that PRP promotes the development of primitive and primary follicles into the presinus stage [104]. Thus, some studies have used AMH as a principal marker to evaluate the efficacy of PRP because AMH levels, which are mainly associated with preantral and antral follicles, appear to be relatively stable across the menstrual cycle [105, 106]. Furthermore, PRP can restore the ovarian microenvironment. More specifically, PRP prevented OS and reduce the oxidation state of the ovary in rat with ovarian ischemia-reperfusion injury [107]. PRP also successfully reduced degeneration and atresia in normal follicles, caused by ovotoxic chemicals, and accelerated angiogenesis [108].

Application of PRP therapy in POI

Clinical application of PRP in human ovaries was first introduced by Pantos et al. [109]. In this study, eight peri-menopausal women were treated with intra-ovarian PRP injections. Their results showed that the menstrual cycle and oocyte retrieval in all patients had recovered following in vitro fertilization (IVF) treatment. However, a small proportion of patients and their previous ovarian reserves were not recorded, limiting the interpretation of these results. In addition, PRP reportedly exerts positive effects on ovarian vascularization. For example, PRP was used during autologous ovarian transplantations to increase the vascular density of grafts [110].

Sfakianoudis et al. (2018) reported that a patient with POI receiving PRP treatment became pregnant following a natural IVF cycle [111]. Sfakianoudis et al. (2020) further reported pilot data pertaining to PRP treatment in POI, which indicated poor ovarian response (POR), peri-menopausal, and menopausal women [99]. The results of this study indicated that the levels of both AMH and AFC were increased while those of FSH and luteinizing hormone were decreased in all patients tested. These research results indicated that PRP therapy effectively restored ovarian functionality and hormonal profile. In another study, researchers evaluated the effect of this therapy on ovarian reserves and IVF outcomes in 311 patients with POI. These results indicated that 23 patients (7.4%) conceived spontaneously after treatment with PRP [102]. In order to improve clinical effect, Chao-Chin et al. injected PRP combined with gonadotropin into the ovarian stroma. Following this treatment, the patient, who had responded poorly to gonadotropins earlier, resumed menstrual periods and achieved successful conception [112].

Risk and countermeasures of PRP therapy

Advantages of autologous PRP intra-ovarian infusion include easy handling, good storage properties, and low immunogenicity. However, the potential risk associated with PRP therapy mainly include infection, intense cell proliferation events, and unknown detrimental effects on the embryo. In terms of infection risk, a few PRP samples were found to be positive for microbial growth [113]. In addition, other adverse events such as infections have been linked to PRP [114]. Therefore, detection and inactivation of blood borne pathogens in samples is vital, despite the fact that some PRP preparations have been found to exhibit antimicrobial properties.

Growth factors derived from PRP govern cell proliferation and differentiation [115]. However, intense cell proliferation events may induce malignancy due to differentiation of stem cells within the ovaries [116]. The final risk associated with this therapy involves detrimental effects exerted on the embryo by high concentrations of hematopoietic cells introduced into the implantation environment by PRP [117]. Thus, further studies are required to provide solid evidence that confirms the safety of PRP therapy.

MicroRNAs: the future direction of POI treatment

MicroRNAs (miRNAs) are short, 18–24 nucleotides long, non-coding RNAs [118]. These regulate cell proliferation, differentiation, and apoptosis in normal and pathological processes [119]. The expression levels of miRNAs in reproductive tissues appears to be linked to fertility potentials and embryo developmental capacities [120]. Furthermore, miRNAs play a regulatory function in folliculogenesis and oocyte maturation [119] and are detected in plasma, serum, and urine. Currently, plasma miRNAs are considered as promising potential biomarkers for a series of cancers and other diseases.

A miRNA microarray analysis conducted by a previous study indicated that 22 miRNAs were significantly upregulated, while 29 were significantly downregulated in POI patients [121]. Several critical miRNAs in POI have been described. MiR-23a and miR-27a are significantly upregulated in the plasma of POI patients [121, 122]. Reportedly, miR-23a induces GC apoptosis by downregulating the X-linked inhibitor of apoptosis proteins and increasing caspase-3 cleavage [122]. These two miRNAs induce GC apoptosis by targeting SMAD5, which activatse the Fas ligand-Fas pathway in vitro [123]. Moreover, a miR-27a mimic sequence transfected into GCs reduced oocyte maturation in mouse follicles [124].

MiR-127-5p is significantly upregulated in the plasma of patients with biochemical POI (bPOI). Biochemical POI refers to elevated FSH levels accompanied by normal menstrual cycle. A study has shown that miR-127-5p inhibits the proliferation of GCs and impairs the ability of DNA damage repair by targeting the POI high mobility group box2 gene [125]. Intriguingly, miR-127-5p was also upregulated in the plasma of bPOI patients, and thus, miR-127-5p has been proposed as a biomarker for bPOI.

Intensive research studies have laid the foundation for using miRNAs in POI therapy. A study found that miRNA-146b-5p overexpression attenuates POI in mice by specifically downregulating p38-Mapk14 and inhibiting γH2A.X phosphorylation. The novelty of this study is that it researched poly (lactic-co-glycolic acid) (PLGA) nanoparticles as a carrier to achieve successful delivery of miRNA-146b-5p. Next, these researchers cultured GCs, derived from mouse POI model, in a medium supplemented with PLGA cross-linked miRNA-146b-5p. The GCs displayed downregulated p38-Mapk14 and alleviated aging.


POI patients have unique needs that require special attention. Different therapeutic strategies that focus on rescuing ovarian function open new opportunities for women with POI. Knowledge regarding various aspects of related fields will enhance the possibilities of treating this disease. Several issues need to be resolved prior to optimization of POI management. Specifically, HRT still remains the central element in the treatment of POI. Clinicians bear responsibility for informing patients that untreated POI may increase the risk for premature death and cardiovascular disease, and should consider the patient’s condition, needs, and preferences during the decision-making process to adjust the formulation, dosage, and duration of use according to individual patient needs. Moreover, an evaluation of the clinical effect exerted by the assigned HRT on the patient needs to be performed.

Although current studies support the development of IVA, this technique is still in its formative stage. Residual follicles form the premise of IVA technology. Therefore, it is necessary to develop novel methods, including imaging techniques such as optical coherence tomography, that help localize residual follicles. In addition, mechanisms underlying fragmentation that disrupts the Hippo pathway, targeting of additional pathways, or other factors that accelerate PF activation, warrant further investigation. Finally, the culturing system of activated follicles should be optimized by incorporating compatible hormonal, paracrine environments and mechanical characteristics.

Currently, due to the scarcity of pertinent studies, strong evidence that demonstrates the effect and safety of mitochondrial activation techniques cannot be produced. Mitochondrial nutrient and transfer therapy continue to be explored. A better understanding of the mechanisms underlying the role played by mitochondrial dysfunction in ovarian aging should be obtained via further research. Revealing the determinants of mitochondrial dysfunction may enhance the development of targeted intervention.

Stem cell therapy has shown promising results against POI. Utilization of exosome replacement cell itself is sufficient to overcome tumorigenesis and immunogenicity of stem cell. Importantly, various biomaterials can be used to deliver stem cell or exosomes, in order to increase the retention and survival rates of stem cells or exosomes in target organs. The future direction of research appears to tilt towards the application of exosomes combined with natural biomaterials. However, in this respect, the biosafety, biodegradation, and biocompatibility of new materials cannot be disregarded.

PRP may be considered as a putative alternative strategy for treating POI. Exhaustive investigation of the safety of this therapy prior to clinical practice is critical. Clinicians offering PRP should confirm platelet and growth factor concentrations, as well as constitution and detection of blood borne pathogens in samples. Moreover, further studies that include appropriate control groups, which help evaluate the efficacy of this technique, should be initiated. The next logical step would be the careful implementation of precisely designed, large scale, randomized clinical trials.

In this review, we propose miRNAs as a potential treatment option for POI. An in-depth understanding of the role of miRNAs in POI would be advantageous in the treatment of ovarian diseases. It is possible to target POI via therapies involving transfected mimics or inhibitors of specific miRNAs. In addition, the prediction and validation of upstream regulators and downstream target genes of miRNAs may also contribute towards the understanding and treatment of POI.

These new therapies will allow clinicians to perform high-quality interventions in the treatment of POI. Notably, a majority of current research on these therapies has been performed on animal models. Considering the vast differences between humans and animals, precise experiments, designed for vertebrates at evolutionary stages varying from lower to higher levels, may ensure that these new technologies can be safely and effectively applied to humans. Furthermore, the sense of balance between patience and caution should be fine-tuned when applying various therapies against POI.

Availability of data and materials

Not applicable.



Primary ovarian insufficiency


Premature ovarian failure


Follicle-stimulating hormone


Anti-Mullerian hormone


Antral follicle count


Hormone replacement therapy


In vitro activation


Platelet-rich plasma


Transdermal patches


Hyaluronic acid


Red blood cells


Primordial follicles


Phosphatase and tensin homolog




Protein kinase B


Forkhead box O3






Phosphatidylinositol-dependent kinase 1


Tuberous sclerosis 2


mammalian target of rapamycin complex


S6 kinase


ribosomal protein S6


4E binding protein 1


Yes-associated protein


Transcriptional co-activator PDZ-binding motif


Baculoviral IAP repeat-containing


Bone morphogenetic proteins


Growth and differentiation factor 9


Granulose cells


Extracellular matrix


mitochondrial DNA


Adenosine triphosphate


Reactive oxygen species


Polymerase gamma


Oxidative stress


Mitofusin 2


Dynamin-related protein 1


Coenzyme Q10


Germinal vesicle


Pronuclear transplantation


Autonomous germline mitochondrial energy transfer


Embryonic stem cells


Adult stem cells


Induced pluripotent stem cells


Mesenchymal stem cells


Human primitive germ-like cells


Bone marrow stem cells


Vascular endothelial growth factor


Cyclin-dependent kinase inhibitor 1A


Bcl-2-associated X protein


Adipose-derived stem cell


Menstrual blood-derived mesenchymal stem cells


Placenta-derived mesenchymal stem cells


Amnion mesenchymal stem cells


Umbilical cord mesenchymal stem cells


Amniotic fluid stem cells


Programmed cell death protein 4


Human leukocyte antigen


In vitro fertilization


Poor ovarian response




biochemical POI


  1. Beck-Peccoz P, Persani L. Premature ovarian failure. Orphanet J rare dis [internet]. Orphanet J Rare Dis. 2006; [cited 2020 Aug 8];1:9. Available from:

  2. Nippita TA, Baber RJ. Premature ovarian failure: A review. Climacteric. Climacteric; 2007;10:11–22.

  3. Lagergren K, Hammar M, Nedstrand E, Bladh M, Sydsjö G. The prevalence of primary ovarian insufficiency in Sweden; A national register study. BMC Womens Health. 2018;18:175.

  4. Golezar S, Ramezani Tehrani F, Khazaei S, Ebadi A, Keshavarz Z. The global prevalence of primary ovarian insufficiency and early menopause: a meta-analysis. Climacteric. 2019;22:403–11.

    CAS  PubMed  Google Scholar 

  5. De Vos M, Devroey P, Fauser BC. Primary ovarian insufficiency. Lancet. 2010;376:911–21.

    PubMed  Google Scholar 

  6. Webber L, Davies M, Anderson R, Bartlett J, Braat D, Cartwright B, et al. ESHRE guideline: management of women with premature ovarian insufficiency. Hum Reprod. 2016;31:926–37.

    CAS  PubMed  Google Scholar 

  7. Rudnicka E, Kruszewska J, Klicka K, Kowalczyk J, Grymowicz M, Skórska J, et al. Premature ovarian insufficiency - aetiopathology, epidemiology, and diagnostic evaluation. Prz Menopauzalny. 2018;17:105–8.

    PubMed  PubMed Central  Google Scholar 

  8. Nelson LM. Clinical practice. Primary ovarian insufficiency. N Engl J Med. 2009;360:606–14 Available from:

    CAS  PubMed  PubMed Central  Google Scholar 

  9. Vo KCT, Kawamura K. In vitro activation early follicles: From the basic science to the clinical perspectives. Int J Mol Sci. 2021;22(7):3785.

  10. Cheng Y, Kim J, Li XX, Hsueh AJ. Promotion of ovarian follicle growth following mTOR activation: Synergistic effects of AKT stimulators. PLoS One. 2015;10(2):e0117769.

  11. Fàbregues F, Ferreri J, Méndez M, Calafell JM, Otero J, Farré R. In Vitro Follicular Activation and Stem Cell Therapy as a Novel Treatment Strategies in Diminished Ovarian Reserve and Primary Ovarian Insufficiency. Front Endocrinol (Lausanne). 2021;11:617704.

  12. Pan D. The hippo signaling pathway in development and cancer. Dev Cell. 2010;19:491–505.

    CAS  PubMed  PubMed Central  Google Scholar 

  13. Lee HN, Chang EM. Primordial follicle activation as new treatment for primary ovarian insufficiency. Clin Exp Reprod Med. 2019;46:43–9.

    PubMed  PubMed Central  Google Scholar 

  14. Kawamura K, Cheng Y, Suzuki N, Deguchi M, Sato Y, Takae S, et al. Hippo signaling disruption and Akt stimulation of ovarian follicles for infertility treatment. Proc Natl Acad Sci U S A. 2013;110:17474–9.

    CAS  PubMed  PubMed Central  Google Scholar 

  15. Ding X, Zhang X, Mu Y, Li Y, Hao J. Effects of BMP4/SMAD signaling pathway on mouse primordial follicle growth and survival via up-regulation of Sohlh2 and c-kit. Mol Reprod Dev. 2013;80:70–8.

    CAS  PubMed  Google Scholar 

  16. Sanfins A, Rodrigues P, Albertini DF. GDF-9 and BMP-15 direct the follicle symphony. J Assist Reprod Genet. 2018;35:1741–50.

    PubMed  PubMed Central  Google Scholar 

  17. Coutts SM, Childs AJ, Fulton N, Collins C, Bayne RAL, McNeilly AS, et al. Activin signals via SMAD2/3 between germ and somatic cells in the human fetal ovary and regulates kit ligand expression. Dev Biol. 2008;314:189–99.

    CAS  PubMed  Google Scholar 

  18. Nilsson E, Rogers N, Skinner MK. Actions of anti-Müllerian hormone on the ovarian transcriptome to inhibit primordial to primary follicle transition. Reproduction. 2007;134:209–21.

    CAS  PubMed  PubMed Central  Google Scholar 

  19. Adhikari D, Gorre N, Risal S, Zhao Z, Zhang H, Shen Y, et al. The safe use of a PTEN inhibitor for the activation of dormant mouse primordial follicles and generation of fertilizable eggs. PLoS One. 2012;7(6):e39034.

  20. Zhang J, Yan L, Wang Y, Zhang S, Xu X, Dai Y, et al. In vivo and in vitro activation of dormant primordial follicles by EGF treatment in mouse and human. Clin Transl Med. 2020;10(5):e182.

  21. Maidarti M, Clarkson YL, Mclaughlin M, Anderson RA, Telfer EE. Inhibition of PTEN activates bovine non-growing follicles in vitro but increases DNA damage and reduces DNA repair response. Hum Reprod. 2019;34:297–307.

    CAS  PubMed  Google Scholar 

  22. Zhang D, Zhang X, Zeng M, Yuan J, Liu M, Yin Y, et al. Increased DNA damage and repair deficiency in granulosa cells are associated with ovarian aging in rhesus monkey. J Assist Reprod Genet. 2015;32:1069–78.

    PubMed  PubMed Central  Google Scholar 

  23. Bertoldo MJ, Walters KA, Ledger WL, Gilchrist RB, Mermillod P, Locatelli Y. In-vitro regulation of primordial follicle activation: challenges for fertility preservation strategies. Reprod BioMed Online. 2018;36:491–9.

    CAS  PubMed  Google Scholar 

  24. McLaughlin M, Innell HL, Anderson RA, Telfer EE. Inhibition of phosphatase and tensin homologue (PTEN) in human ovary in vitro results in increased activation of primordial follicles but compromises development of growing follicles. Mol Hum Reprod. 2014;20:736–44.

    CAS  PubMed  PubMed Central  Google Scholar 

  25. Cheng Y, Feng Y, Jansson L, Sato Y, Deguchi M, Kawamura K, et al. Actin polymerization-enhancing drugs promote ovarian follicle growth mediated by the hippo signaling effector YAP. FASEB J. 2015;29:2423–30.

    CAS  PubMed  PubMed Central  Google Scholar 

  26. Shah JS, Sabouni R, Cayton Vaught KC, Owen CM, Albertini DF, Segars JH. Biomechanics and mechanical signaling in the ovary: a systematic review. J Assist Reprod Genet. 2018;35:1135–48.

    PubMed  PubMed Central  Google Scholar 

  27. Nagamatsu G, Shimamoto S, Hamazaki N, Nishimura Y, Hayashi K. Mechanical stress accompanied with nuclear rotation is involved in the dormant state of mouse oocytes. Sci Adv. 2019;5(6):eaav9960.

  28. Ouni E, Bouzin C, Dolmans MM, Marbaix E, Pyr Dit Ruys S, Vertommen D, et al. Spatiotemporal changes in mechanical matrisome components of the human ovary from prepuberty to menopause. Hum Reprod. 2020;35:1391–410.

    CAS  PubMed  Google Scholar 

  29. Zhai J, Yao G, Dong F, Bu Z, Cheng Y, Sato Y, et al. In vitro activation of follicles and fresh tissue auto-transplantation in primary ovarian insufficiency patients. J Clin Endocrinol Metab. 2016;101:4405–12.

    CAS  PubMed  PubMed Central  Google Scholar 

  30. Kawamura K, Ishizuka B, Hsueh AJW. Drug-free in-vitro activation of follicles for infertility treatment in poor ovarian response patients with decreased ovarian reserve. Reprod BioMed Online. 2020;40:245–53.

    CAS  PubMed  Google Scholar 

  31. Ferreri J, Fàbregues F, Calafell JM, Solernou R, Borrás A, Saco A, et al. Drug-free in-vitro activation of follicles and fresh tissue autotransplantation as a therapeutic option in patients with primary ovarian insufficiency. Reprod BioMed Online. 2020;40:254–60.

    CAS  PubMed  Google Scholar 

  32. Resetkova N, Hayashi M, Kolp LA, Christianson MS. Fertility preservation for Prepubertal girls: update and current challenges. Curr Obstet Gynecol Rep. 2013;2:218–25.

    PubMed  PubMed Central  Google Scholar 

  33. De Roo C, Lierman S, Tilleman K, De Sutter P. In-vitro fragmentation of ovarian tissue activates primordial follicles through the Hippo pathway . Hum Reprod Open. 2020;2020(4):hoaa048.

  34. Gavish Z, Spector I, Peer G, Schlatt S, Wistuba J, Roness H, et al. Follicle activation is a significant and immediate cause of follicle loss after ovarian tissue transplantation. J Assist Reprod Genet. 2018;35:61–9.

    PubMed  Google Scholar 

  35. Benkhalifa M, Ferreira YJ, Chahine H, Louanjli N, Miron P, Merviel P, et al. Mitochondria: participation to infertility as source of energy and cause of senescence. Int J Biochem Cell Biol. 2014;55:60–4.

    CAS  PubMed  Google Scholar 

  36. Duran HE, Simsek-Duran F, Oehninger SC, Jones HW, Castora FJ. The association of reproductive senescence with mitochondrial quantity, function, and DNA integrity in human oocytes at different stages of maturation. Fertil Steril. 2011;96:384–8.

    CAS  PubMed  Google Scholar 

  37. Wang T, Zhang M, Jiang Z, Seli E. Mitochondrial dysfunction and ovarian aging. Am J Reprod Immunol. 2017;77:5.

  38. May-Panloup P, Chrétien MF, Jacques C, Vasseur C, Malthièry Y, Reynier P. Low oocyte mitochondrial DNA content in ovarian insufficiency. Hum Reprod. 2005;20:593–7.

    CAS  PubMed  Google Scholar 

  39. Meldrum DR, Casper RF, Diez-Juan A, Simon C, Domar AD, Frydman R. Aging and the environment affect gamete and embryo potential: can we intervene? Fertil Steril. 2016;105:548–59.

    PubMed  Google Scholar 

  40. Latorre-Pellicer A, Moreno-Loshuertos R, Lechuga-Vieco AV, Sánchez-Cabo F, Torroja C, Acín-Pérez R, et al. Mitochondrial and nuclear DNA matching shapes metabolism and healthy ageing. Nature. 2016;535:561–5.

    CAS  PubMed  Google Scholar 

  41. Konstantinidis M, Alfarawati S, Hurd D, Paolucci M, Shovelton J, Fragouli E, et al. Simultaneous assessment of aneuploidy, polymorphisms, and mitochondrial DNA content in human polar bodies and embryos with the use of a novel microarray platform. Fertil Steril. 2014;102:1385–92.

    CAS  PubMed  Google Scholar 

  42. Kumar M, Pathak D, Kriplani A, Ammini AC, Talwar P, Dada R. Nucleotide variations in mitochondrial DNA and supra-physiological ROS levels in cytogenetically normal cases of premature ovarian insufficiency. Arch Gynecol Obstet. 2010;282:695–705.

    CAS  PubMed  Google Scholar 

  43. Kasapoǧlu I, Seli E. Mitochondrial Dysfunction and Ovarian Aging. Endocrinol (United States). 2020;161(2):undefined.

  44. He Q, Gu L, Lin Q, Ma Y, Liu C, Pei X, et al. The Immp2l Mutation Causes Ovarian Aging through ROS-Wnt/β-Catenin-Estrogen Pathway: Preventive Effect of Melatonin. Endocrinol (United States). 2020;161(9):undefined

  45. Zhang M, Bener MB, Jiang Z, Wang T, Esencan E, Scott R, et al. Mitofusin 2 plays a role in oocyte and follicle development, and is required to maintain ovarian follicular reserve during reproductive aging. Aging (Albany NY). 2019;11:3919–38.

    CAS  Google Scholar 

  46. Udagawa O, Ishihara T, Maeda M, Matsunaga Y, Tsukamoto S, Kawano N, et al. Mitochondrial fission factor Drp1 maintains oocyte quality via dynamic rearrangement of multiple organelles. Curr Biol. 2014;24:2451–8.

    CAS  PubMed  Google Scholar 

  47. Gispert S, Parganlija D, Klinkenberg M, Dröse S, Wittig I, Mittelbronn M, et al. Loss of mitochondrial peptidase clpp leads to infertility, hearing loss plus growth retardation via accumulation of CLPX, mtDNA and inflammatory factors. Hum Mol Genet. 2013;22:4871–87.

    CAS  PubMed  Google Scholar 

  48. Liu MJ, Sun AG, Zhao SG, Liu H, Ma SY, Li M, et al. Resveratrol improves in vitro maturation of oocytes in aged mice and humans. Fertil Steril. 2018;109:900–7.

    CAS  PubMed  Google Scholar 

  49. Ben-Meir A, Burstein E, Borrego-Alvarez A, Chong J, Wong E, Yavorska T, et al. Coenzyme Q10 restores oocyte mitochondrial function and fertility during reproductive aging. Aging Cell. 2015;14:887–95.

    CAS  PubMed  PubMed Central  Google Scholar 

  50. Bentov Y, Hannam T, Jurisicova A, Esfandiari N, Casper RF. Coenzyme Q10 supplementation and oocyte aneuploidy in women undergoing IVF-ICSI treatment. Clin Med Insights Reprod Heal. 2014;8:CMRH.S14681.

    Google Scholar 

  51. Liu M, Yin Y, Ye X, Zeng M, Zhao Q, Keefe DL, et al. Resveratrol protects against age-associated infertility in mice. Hum Reprod. 2013;28:707–17.

    CAS  PubMed  Google Scholar 

  52. Ochiai A, Kuroda K. Preconception resveratrol intake against infertility: friend or foe? Reprod Med Biol. 2020;19:107–13.

    CAS  PubMed  Google Scholar 

  53. Tamura H, Kawamoto M, Sato S, Tamura I, Maekawa R, Taketani T, et al. Long-term melatonin treatment delays ovarian aging. J Pineal Res. 2017;62(2):undefined.

  54. Cohen J, Scott R, Schimmel T, Levron J, Willadsen S. Birth of infant after transfer of anucleate donor oocyte cytoplasm into recipient eggs [5]. Lancet. 1997;350:186–7.

    CAS  PubMed  Google Scholar 

  55. Barritt JA, Brenner CA, Malter HE, Cohen J. Mitochondria in human offspring derived from ooplasmic transplantation. Hum Reprod. 2001;16:513–6.

    CAS  PubMed  Google Scholar 

  56. Zhang J, Liu H, Luo S, Lu Z, Chávez-Badiola A, Liu Z, et al. Live birth derived from oocyte spindle transfer to prevent mitochondrial disease. Reprod BioMed Online. 2017;34:361–8.

    PubMed  Google Scholar 

  57. Zhang J. Revisiting germinal vesicle transfer as a treatment for aneuploidy in infertile women with diminished ovarian reserve. J Assist Reprod Genet. 2015;32:313–7.

    PubMed  Google Scholar 

  58. Ishii T, Hibino Y. Mitochondrial manipulation in fertility clinics: regulation and responsibility. Reprod Biomed Soc Online. 2018;5:93–109.

    PubMed  PubMed Central  Google Scholar 

  59. Cecchino GN, Seli E, Alves da Motta EL, García-Velasco JA. The role of mitochondrial activity in female fertility and assisted reproductive technologies: overview and current insights. Reprod BioMed Online. 2018;36:686–97.

    CAS  PubMed  Google Scholar 

  60. Oktay K, Baltaci V, Sonmezer M, Turan V, Unsal E, Baltaci A, et al. Oogonial precursor cell-derived autologous mitochondria injection to improve outcomes in women with multiple IVF failures due to low oocyte quality: a clinical translation. Reprod Sci. 2015;22:1612–7.

    PubMed  Google Scholar 

  61. Labarta E, de los Santos MJ, Herraiz S, Escribá MJ, Marzal A, Buigues A, et al. Autologous mitochondrial transfer as a complementary technique to intracytoplasmic sperm injection to improve embryo quality in patients undergoing in vitro fertilization—a randomized pilot study. Fertil Steril. 2019;111:86–96.

    PubMed  Google Scholar 

  62. Kolios G, Moodley Y. Introduction to stem cells and regenerative medicine. Respiration. 2012;85:3–10.

    PubMed  Google Scholar 

  63. Na J, Kim GJ. Recent trends in stem cell therapy for premature ovarian insufficiency and its therapeutic potential: a review. J Ovarian Res. 2020;13:1–10.

    Google Scholar 

  64. Zhao YX, Chen SR, Su PP, Huang FH, Shi YC, Shi QY, et al. Using Mesenchymal Stem Cells to Treat Female Infertility: An Update on Female Reproductive Diseases. Stem Cells Int. 2019;2019:9071720.

  65. Davis ME. Exosomes: what do we love so much about them? Circ Res. 2016;119:1280–2 Available from:

    CAS  PubMed  PubMed Central  Google Scholar 

  66. Zhai M, Zhu Y, Yang M, Mao C. Human mesenchymal stem cell derived exosomes enhance cell-free bone regeneration by altering their miRNAs profiles. Adv Sci. 2020;2001334:1–15.

    Google Scholar 

  67. Wang ZB, Hao JX, Meng TG, Guo L, Dong MZ, Fan LH, et al. Transfer of autologous mitochondria from adipose tissue-derived stem cells rescues oocyte quality and infertility in aged mice. Aging. 2017;9:2480–8.

    CAS  PubMed  PubMed Central  Google Scholar 

  68. Esfandyari S, Chugh RM, Park HS, Hobeika E, Ulin M, Al-Hendy A. Mesenchymal stem cells as a bio organ for treatment of female infertility. Cells. 2020;9:1–19.

    Google Scholar 

  69. Yamashiro C, Sasaki K, Yokobayashi S, Kojima Y, Saitou M. Generation of human oogonia from induced pluripotent stem cells in culture. Nat Protoc. 2020;15:1560–83.

    CAS  PubMed  Google Scholar 

  70. Abd-Allah SH, Shalaby SM, Pasha HF, El-Shal AS, Raafat N, Shabrawy SM, et al. Mechanistic action of mesenchymal stem cell injection in the treatment of chemically induced ovarian failure in rabbits. Cytotherapy. 2013;15:64–75.

    CAS  PubMed  Google Scholar 

  71. Guo J qi, Gao X, Lin Z jie, Wu W zhen, Huang L hu, Dong H yue, et al. BMSCs reduce rat granulosa cell apoptosis induced by cisplatin and perimenopause. BMC Cell Biol. 2013;14:18.

  72. Terraciano P, Garcez T, Ayres L, Durli I, Baggio M, Kuhl CP, et al. Cell therapy for chemically induced ovarian failure in mice. Stem Cells Int. Hindawi Publishing Corporation. 2014;2014:720753.

  73. Yan Z, Guo F, Yuan Q, Shao Y, Zhang Y, Wang H, et al. Endometrial mesenchymal stem cells isolated from menstrual blood repaired epirubicin-induced damage to human ovarian granulosa cells by inhibiting the expression of Gadd45b in cell cycle pathway. Stem Cell Res Ther. 2019;10:4. 

  74. Wang Z, Wang Y, Yang T, Li J, Yang X. Study of the reparative effects of menstrual-derived stem cells on premature ovarian failure in mice. Stem Cell Res Ther. 2017;8:1–14.

  75. Zhang H, Luo Q, Lu X, Yin N, Zhou D, Zhang L, et al. Effects of hPMSCs on granulosa cell apoptosis and AMH expression and their role in the restoration of ovary function in premature ovarian failure mice. Stem Cell Res Ther. 2018;9:20.

  76. Yin N, Wang Y, Lu X, Liu R, Zhang L, Zhao W, et al. HPMSC transplantation restoring ovarian function in premature ovarian failure mice is associated with change of Th17/Tc17 and Th17/Treg cell ratios through the PI3K/Akt signal pathway. Stem Cell Res Ther. Stem Cell Res Ther. 2018;9:1–14.

  77. Seok J, Park H, Choi JH, Lim JY, Kim KG, Kim GJ. Placenta‐derived mesenchymal stem cells restore the ovary function in an ovariectomized rat model via an antioxidant effect. Antioxidants. 2020;9:1–16.

  78. Li H, Zhao W, Wang L, Luo Q, Yin N, Lu X, et al. Human placenta-derived mesenchymal stem cells inhibit apoptosis of granulosa cells induced by IRE1α pathway in autoimmune POF mice. Cell Biol Int. 2019;43:899–909.

  79. Cui L, Bao H, Liu Z, Man X, Liu H, Hou Y, et al. HUMSCs regulate the differentiation of ovarian stromal cells via TGF-β1/Smad3 signaling pathway to inhibit ovarian fibrosis to repair ovarian function in POI rats. Stem Cell Res Ther. 2020;11:386.

  80. Yu X, Wang N, Qiang R, Wan Q, Qin M, Chen S, et al. Human amniotic fluid stem cells possess the potential to differentiate into primordial follicle oocytes in vitro. Biol Reprod. 2014;90(4):73, 1–11.

  81. Ling L, Feng X, Wei T, Wang Y, Wang Y, Zhang W, et al. Effects of low-intensity pulsed ultrasound (LIPUS)-pretreated human amnion-derived mesenchymal stem cell (hAD-MSC) transplantation on primary ovarian insufficiency in rats. Stem Cell Res Ther. 2017;8:283. 

  82. Sun B, Ma Y, Wang F, Hu L, Sun Y. miR-644-5p carried by bone mesenchymal stem cell-derived exosomes targets regulation of p53 to inhibit ovarian granulosa cell apoptosis. Stem Cell Res Ther. Stem Cell Research & Therapy; 2019;10:1–9.

  83. Yang M, Lin L, Sha C, Li T, Zhao D, Wei H, et al. Bone marrow mesenchymal stem cell-derived exosomal miR-144-5p improves rat ovarian function after chemotherapy-induced ovarian failure by targeting PTEN. Lab Investig. 2020;100:342–52.

  84. Fu X, He Y, Wang X, Peng D, Chen X, Li X, et al. Overexpression of miR-21 in stem cells improves ovarian structure and function in rats with chemotherapy-induced ovarian damage by targeting PDCD4 and PTEN to inhibit granulosa cell apoptosis. Stem Cell Res Ther. 2017;8:187.

  85. Huang B, Lu J, Ding C, Zou Q, Wang W, Li H. Exosomes derived from human adipose mesenchymal stem cells improve ovary function of premature ovarian insufficiency by targeting SMAD. Stem Cell Res Ther. 2018;9:216.

  86. Ding C, Zhu L, Shen H, Lu J, Zou Q, Huang C, et al. Exosomal miRNA-17-5p derived from human umbilical cord mesenchymal stem cells improves ovarian function in premature ovarian insufficiency by regulating SIRT7. Stem Cells. 2020;38:1137–48.

  87. Xiao GY, Cheng CC, Chiang YS, Cheng WTK, Liu IH, Wu SC. Exosomal miR-10a derived from amniotic fluid stem cells preserves ovarian follicles after chemotherapy. Sci Rep. 2016;6:23120.

  88. Ding C, Qian C, Hou S, Lu J, Zou Q, Li H, et al. Exosomal miRNA-320a Is Released from hAMSCs and Regulates SIRT4 to Prevent Reactive Oxygen Species Generation in POI. Mol Ther - Nucleic Acids [Internet]. Elsevier Ltd.; 2020;21:37–50. Available from:

  89. Su J, Ding L, Cheng J, Yang J, Li X, Yan G, et al. Transplantation of adipose-derived stem cells combined with collagen scaffolds restores ovarian function in a rat model of premature ovarian insufficiency. Hum Reprod. 2016;31:1075–86.

  90. Ding L, Yan G, Wang B, Xu L, Gu Y, Ru T, et al. Transplantation of UC-MSCs on collagen scaffold activates follicles in dormant ovaries of POF patients with long history of infertility. Sci China Life Sci. 2018;61:1554–65.

  91. Green LJ, Zhou H, Padmanabhan V, Shikanov A. Adipose-derived stem cells promote survival , growth , and maturation of early- stage murine follicles. Stem Cell Res Ther. 2019;8:1–13.

  92. He X. Microfluidic Encapsulation of Ovarian Follicles for 3D Culture. Ann Biomed Eng. 2017;45:1676–84.

  93. Amorim CA, Van Langendonckt A, David A, Dolmans MM, Donnez J. Survival of human pre-antral follicles after cryopreservation of ovarian tissue, follicular isolation and in vitro culture in a calcium alginate matrix. Hum Reprod. 2009;24:92–9.

  94. Kim H, Shin M, Han S, Kwon W, Hahn SK. Hyaluronic acid derivatives for translational medicines. Biomacromolecules. 2019;20:2889–903.

    CAS  PubMed  Google Scholar 

  95. Zhao G, Zhou X, Fang T, Hou Y, Hu Y. Hyaluronic acid promotes the expression of progesterone receptor membrane component 1 via epigenetic silencing of miR-139-5p in human and rat granulosa cells. Biol Reprod. 2014;91(5):116, 1–9.

  96. Yamanaka S. Pluripotent stem cell-based cell therapy—promise and challenges. Cell Stem Cell. 2020;27:523–31.

    CAS  PubMed  Google Scholar 

  97. Yin JQ, Zhu J, Ankrum JA. Manufacturing of primed mesenchymal stromal cells for therapy. Nat Biomed Eng. 2019;3:90–104. Springer US.

    CAS  PubMed  Article  Google Scholar 

  98. Bos-Mikich A, De OR, Frantz N. Platelet-rich plasma therapy and reproductive medicine. J Assist Reprod Genet. 2018;35:753–6.

    PubMed  PubMed Central  Google Scholar 

  99. Sfakianoudis K, Simopoulou M, Grigoriadis S, Pantou A, Tsioulou P, Maziotis E, et al. Reactivating ovarian function through autologous platelet-rich plasma Intraovarian infusion: pilot data on premature ovarian insufficiency, Perimenopausal, menopausal, and poor responder women. J Clin Med. 2020;9:1809.

    PubMed Central  Google Scholar 

  100. Chen L, Qu J, Xiang C. The multi-functional roles of menstrual blood-derived stem cells in regenerative medicine. Stem Cell Res Ther. 2019;10:1.

  101. Sundman EA, Cole BJ, Karas V, Della Valle C, Tetreault MW, Mohammed HO, et al. The anti-inflammatory and matrix restorative mechanisms of platelet-rich plasma in osteoarthritis. Am J Sports Med. 2014;42:35–41.

    PubMed  Google Scholar 

  102. Cakiroglu Y, Saltik A, Yuceturk A, Karaosmanoglu O, Kopuk SY, Scott RT, et al. Effects of intraovarian injection of autologous platelet rich plasma on ovarian reserve and IVF outcome parameters in women with primary ovarian insufficiency. Aging. 2020;12:10211–22.

    CAS  PubMed  PubMed Central  Google Scholar 

  103. Sfakianoudis K, Simopoulou M, Nitsos N, Rapani A, Pappas A, Pantou A, et al. Autologous platelet-rich plasma treatment enables pregnancy for a woman in premature menopause. J Clin Med. 2018;8:1.

    PubMed Central  Google Scholar 

  104. Hosseini L, Shirazi A, Naderi MM, Shams-Esfandabadi N, Borjian Boroujeni S, Sarvari A, et al. Platelet-rich plasma promotes the development of isolated human primordial and primary follicles to the preantral stage. Reprod Biomed. 2017;35:343–50: . Elsevier ltd.

    CAS  Article  Google Scholar 

  105. Jeppesen JV, Anderson RA, Kelsey TW, Christiansen SL, Kristensen SG, Jayaprakasan K, et al. Which follicles make the most anti-Mü llerian hormone in humans? Evidence for an abrupt decline in AMH production at the time of follicle selection. Mol Hum Reprod. 2013;19:519–27.

    CAS  PubMed  Google Scholar 

  106. Gracia CR, Shin SS, Prewitt M, Chamberlin JS, Lofaro LR, Jones KL, et al. Multi-center clinical evaluation of the access amh assay to determine amh levels in reproductive age women during normal menstrual cycles. J Assist Reprod Genet. 2018;35:777–83.

    PubMed  PubMed Central  Google Scholar 

  107. Bakacak M, Bostanci MS, Inanc F, Yaylali A, Serin S, Attar R, et al. Protective effect of platelet rich plasma on experimental ischemia/reperfusion injury in rat ovary. Gynecol Obstet Investig. 2016;81:225–31.

    CAS  Google Scholar 

  108. Ahmadian S, Sheshpari S, Pazhang M, Bedate AM, Beheshti R, Abbasi MM, et al. Intra-ovarian injection of platelet-rich plasma into ovarian tissue promoted rejuvenation in the rat model of premature ovarian insufficiency and restored ovulation rate via angiogenesis modulation. Reprod biol Endocrinol. Reprod Biol Endocrinol. 2020;18:1–13.

    Google Scholar 

  109. Pantos K, Nitsos N, Kokkali G, Vaxevanoglou T, Markomichali C, Pantou A, et al. Ovarian rejuvenation and folliculogenesis reactivation in peri-menopausal women after autologous platelet-rich plasma treatment. Hum Reprod. 2016;31:i301 Available from:

    Google Scholar 

  110. Callejo J, Salvador C, González-Nuñez S, Almeida L, Rodriguez L, Marqués L, et al. Live birth in a woman without ovaries after autograft of frozen-thawed ovarian tissue combined with growth factors. J Ovarian Res. 2013;6:33.

  111. Sfakianoudis K, Simopoulou M, Nitsos N, Rapani A, Pappas A, Pantou A, et al. Autologous Platelet-Rich Plasma Treatment Enables Pregnancy for a Woman in Premature Menopause. J Clin Med. 2018;8:1–7.

  112. Hsu CC, Hsu L, Hsu I, Chiu YJ, Dorjee S. Live birth in woman with premature ovarian insufficiency receiving ovarian Administration of Platelet-Rich Plasma (PRP) in combination with gonadotropin: a case report. Front Endocrinol (Lausanne). 2020;11:1–5.

    Google Scholar 

  113. Reurink G, Goudswaard GJ, Moen MH, Weir A, Verhaar JAN, Bierma-Zeinstra SMA, et al. Rationale, secondary outcome scores and 1-year follow-up of a randomised trial of platelet-rich plasma injections in acute hamstring muscle injury: the Dutch hamstring injection therapy study. Br J Sports Med. 2015;49:1206–12.

    PubMed  Google Scholar 

  114. Schepull T, Kvist J, Norrman H, Trinks M, Berlin G, Aspenberg P. Autologous platelets have no effect on the healing of human Achilles tendon ruptures: a randomized single-blind study. Am J Sports Med. 2011;39:38–47.

    PubMed  Google Scholar 

  115. Liao HT, James IB, Marra KG, Rubin JP. The effects of platelet-rich plasma on cell proliferation and Adipogenic potential of adipose-derived stem cells. Tissue Eng - Part A. 2015;21:2714–22.

    CAS  PubMed  PubMed Central  Google Scholar 

  116. Scott Sills E, Wood SH. Autologous activated platelet-rich plasma injection into adult human ovary tissue: Molecular mechanism, analysis, and discussion of reproductive response. Biosci Rep. 2019;39(6): BSR20190805.

  117. Urman B, Boza A, Balaban B. Platelet-rich plasma another add-on treatment getting out of hand? How can clinicians preserve the best interest of their patients? Hum Reprod. 2019;34:2099–103.

    CAS  PubMed  Google Scholar 

  118. Zhang J, Xu Y, Liu H, Pan Z. MicroRNAs in ovarian follicular atresia and granulosa cell apoptosis. Reprod Biol Endocrinol. 2019;17:9.

  119. Imbar T, Eisenberg I. Regulatory role of microRNAs in ovarian function. Fertil Steril. 2014;101:1524–30.

    CAS  PubMed  Google Scholar 

  120. Salas-Huetos A, James ER, Aston KI, Jenkins TG, Carrell DT, Yeste M. The expression of miRNAs in human ovaries, oocytes, extracellular vesicles, and early embryos: a systematic review. Cells. 2019;8(12):1564.

  121. Dang Y, Zhao S, Qin Y, Han T, Li W, Chen ZJ. MicroRNA-22-3p is down-regulated in the plasma of Han Chinese patients with premature ovarian failure. Fertil Steril. 2015;103:802–807.e1.

    CAS  PubMed  Google Scholar 

  122. Yang X, Zhou Y, Peng S, Wu L, Lin HY, Wang S, et al. Differentially expressed plasma microRNAs in premature ovarian failure patients and the potential regulatory function of mir-23a in granulosa cell apoptosis. Reproduction. 2012;144:234–44.

    Google Scholar 

  123. Nie M, Yu S, Peng S, Fang Y, Wang H, Yang X. miR-23a and miR-27a promote human granulosa cell apoptosis by targeting SMAD51. Biol Reprod. 2015;93(4):98, 1–10.

  124. Kim YJ, Ku SY, Kim YY, Liu HC, Chi SW, Kim SH, et al. MicroRNAs transfected into granulosa cells may regulate oocyte meiotic competence during in vitro maturation of mouse follicles. Hum Reprod. 2013;28:3050–61.

    CAS  PubMed  Google Scholar 

  125. Zhang X, Dang Y, Liu R, Zhao S, Ma J, Qin Y. MicroRNA-127-5p impairs function of granulosa cells via HMGB2 gene in premature ovarian insufficiency. J Cell Physiol. 2020;235:8826–38.

    CAS  PubMed  Google Scholar 

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We thank The Second Affiliated Hospital of Fujian Medical University for its support. We would also like to thank Editage for English language editing.


This work was supported by Science and Technology Bureau of Quanzhou (grant number 2020CT003).

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QH, SL and QS contributed to the conception and design of the review. QH drafted and finalized the manuscript. SL and QS contributed equally to writing the review. SL and QS revised the manuscript and provided critical advice on the content of the manuscript. All authors have read and agreed to the published version of the manuscript.

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Correspondence to Qi-yang Shi or Shu Lin.

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Huang, Qy., Chen, Sr., Chen, Jm. et al. Therapeutic options for premature ovarian insufficiency: an updated review. Reprod Biol Endocrinol 20, 28 (2022).

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  • Premature ovarian insufficiency
  • Therapeutic options
  • Stem cell therapy
  • In vitro activation
  • Mitochondrial activation technique
  • Platelet rich plasma