Abstract
Molecular pathology and genetics are the subjects of increasing focus since they are providing a link between etiologic factors and the heterogeneity of clinicopathologic manifestations that have been covered in the preceding chapters. In endometrial cancer, two divergent pathways have been delineated that may be thought as analogous to the hormone-dependent and -independent subtypes in cancers of breast and prostate. Most hormone dependent EC are EEC, which from a molecular point of view can be classified into different subgroups: (a) ultramutated, due to POLE mutations; (b) hypermutated tumors with MSI, most frequently due to MLH1 promoter, but also seen in Lynch syndrome; and (c) MSS EC with low mutation rate, the most frequent subgroup of EEC. Hormone-independent tumors are represented by serous carcinomas, characterized by a high rate of mutations in p53 that produce genomic instability with extensive somatic copy number alterations. Knowledge on alterations in sarcomas will hopefully lead to advances in diagnosis and therapy that are urgently needed in women where spread beyond the uterus has occurred.
The original version of this chapter was revised. An erratum to this chapter can be found at DOI 10.1007/7631_2018_3
Access provided by CONRICYT-eBooks. Download chapter PDF
Similar content being viewed by others
Keywords
Endometrial Carcinoma
Molecular Abnormalities
During the last few years, it has been demonstrated that endometrioid (EEC) (type I) and non-endometrioid (type II) endometrial carcinomas (NEEC) not only differed from epidemiologic, clinical, and morphologic viewpoints but also regarding molecular alterations implicated in their initiation and progression. Several different molecular pathways are involved in EEC development, including DNA mismatch repair (MMR), phosphoinositide 3-kinase (PI3K)/Akt, RAS-RAF-MEK-ERK, fibroblast growth factor (FGF), and WNT pathways. Alterations in some of these pathways have also been found in atypical endometrial hyperplasia, indicating their role in tumor initiation, but they are infrequent in NECC. In contrast, TP53 mutations occur in a high percentage of NEEC, mainly in serous carcinomas and in its precursor lesion, endometrial intraepithelial carcinoma, but are detected only in a subset of grade 3 EECs. In addition, it has been suggested that TP53 inactivation may be implicated in the phenotypic change from EEC to NEEC as observed in some mixed carcinomas [1, 2] (Table 1).
Recently, the Cancer Genome Atlas Research Network (TCGA) [2] proposed a new molecular classification of endometrial cancer (EC). Based on a combination of somatic mutations, microsatellite instability (MSI), and somatic copy number variations, the endometrial tumors were classified into four groups: (1) an ultra-mutated group with unusually high mutation rates; (2) a hypermutated group with microsatellite instability (MSI), most with MLH1 promoter methylation; (3) a group with lower mutation frequency and most of the microsatellite stable (MSS) endometrioid cancers; and (4) a group that consists primarily of serous-like cancers with extensive somatic copy number alterations and a low mutation rate. Groups 1, 2, and 3 included predominantly endometrioid carcinomas, whereas group 4 included serous carcinomas and some grade 3 endometrioid carcinomas.
POLE Mutations
The ultra-mutated group of EC is characterized by mutations in the exonuclease domain of POLE, which is a catalytic subunit of DNA polymerase epsilon involved in nuclear DNA replication and repair [3]. Seventy five percent of mutations are located at hot-spots P286R and V411L. Ultra-mutated tumors represented 7 % of EC in the TCGA series and showed an increased C → A transversion frequency [2]. The majority demonstrated defining morphological features of endometrioid differentiation, they were frequently high grade (60 %) and rich in tumor-infiltrating lymphocytes and/or peri-tumoral lymphocytes (84 %); many tumors showed morphological heterogeneity (52 %) and ambiguity (16 %). Foci demonstrating severe nuclear atypia led to concern for serous carcinoma in 28 % of the tumors [4].
At the molecular level, the majority of the TCGA POLE-mutated tumors were microsatellite stable (65 %), and TP53 mutations were present in 35 % of them. They also harbored mutations in PTEN (94 %), FBXW7 (82 %), ARID1A (76 %), and PIK3CA (71 %). Since all patients in TCGA and other cohorts [4, 5] were alive without disease, it has been suggested that ultra-mutated tumors have an excellent prognosis despite of adverse molecular and pathological features. However, other authors have not found POLE mutations as prognostic factor in EC [6]. Some studies have demonstrated that POLE mutations may induce MSI by generating somatic mutations in DNA mismatch repair genes, most frequently in MSH6, in a subset of tumors. Thus, POLE testing in MSI ECs could serve as a marker of somatic disease origin and therefore, may be a valuable exclusionary criterion for Lynch syndrome gene testing [6, 7].
DNA Mismatch Repair Deficiency
Microsatellite instability represents a pattern of mutations in cells with a replication error phenotype due to deficient DNA MMR. Microsatellite loci contain repetitive elements of 1–6 nucleotides in length and are most commonly (CA) or poly A/T sequences. MSI status can be detected by using a standard panel of five microsatellite markers. When at least two of the five markers show MSI, tumors are classified as MSI-high (MSI-H). In contrast, tumors without size alteration in microsatellites or those with only one altered marker are classified as microsatellite stable (MSS) and MSI-low (MSI-L), respectively. From a clinicopathologic point of view, MSI-L tumors should be included with MSS tumors [8]. Microsatellite instability was first reported in colorectal adenocarcinomas of patients with Lynch syndrome (hereditary nonpolyposis colorectal cancer, HNPCC). This status of high-frequency mutagenesis is caused by mutations in the main DNA MMR genes, such as hMLH1 and hMSH2 and less frequently hMSH6, hPMS1, and hPMS2. MSI is also seen in approximately 15 % of sporadic colorectal carcinomas, usually reflecting loss of expression of hMLH1 associated with gene silencing by hMLH1 promoter methylation [9].
Available data indicate that EC is the most common extracolonic tumor in Lynch syndrome, with lifetime risk estimates ranging from 40 to 60 % in female mutation carriers [10]. As a result, the original Amsterdam criteria for Lynch syndrome were revised in 1999 to include EC among the diagnostic criteria [11]. It has been suggested that EC is the most common malignancy among women carrying hMSH6 germ line mutations [12].
MSI is seen in approximately 15–45 % of sporadic EEC [13], usually reflecting loss of expression of hMLH1 associated with gene silencing by hMLH1 promoter methylation. This change has been reported in 69–92 % of EC with MSI [14, 15]. In addition, it has been shown that the hMLH1 promoter is frequently methylated in the histologically normal endometrium [15] and atypical endometrial hyperplasia [14] of patients with ECs and that the methylation status is similar to that in the carcinoma. These findings support the notion that, in a subset of tumors, epigenetic changes in DNA MMR genes might be the initial events that trigger the genetic alterations involved in endometrial carcinogenesis.
Immunohistochemistry can be used to explore MMR gene inactivation in EC. Currently, there are antibodies available to study the expression of the most important MMR proteins, such as hMLH1, hMSH2, hMSH6, and hPMS2. In colon cancer, large studies comparing immunohistochemistry and MSI genotyping have demonstrated a 93–100 % sensitivity to detect MSI by immunohistochemistry analysis. Although there are not such large series in EC, different studies have reported a 70–100 % sensitivity when using immunohistochemistry (Fig. 1) [16, 17].
MMR deficiency in cancer produces instability not only in microsatellites that are located in noncoding sequences, such as those used for MSI genotyping, but also in mononucleotide tract repeats located in coding sequences of different genes. The proteins encoded by these genes participate in a variety of essential cellular processes like signal transduction (TGFβRII, IGFIIR, PTEN), apoptosis (BAX), DNA repair (hMSH3, hMSH6, MBD4), transcriptional regulation (TCF-4), protein translocation and modification (SEC63, OGT), or immune surveillance (β2M). It is generally believed that this subset of critical targets specifically promotes MSI carcinogenesis in a large proportion of tumors. Moreover, several studies have demonstrated that selection of target gene mutations in MSI cancers is a tissue-specific process. Whereas some of the genes were proposed to be real target genes for mutation in the most common types of cancers with MSI (colon, gastric, and endometrial cancer) (TGFβRII, BAX, IGFIIR, MSH3, MSH6, and GRB14), selection of other genes for mutation appeared to be dependent on the primary site of the tumor. ECs with MSI accumulate significantly fewer mutations at coding repeats compared to gastrointestinal MSI tumors. For example, the almost systematic TGFβRII gene mutation in MSI gastrointestinal tumors was observed in only 0–10 % of the MSI EC in different series [18,19,20].
Although MSI occurs in a substantial fraction of sporadic EC, data on whether these endometrial tumors differ from their MSI-negative counterparts in clinical characteristics, pathologic features, and survival is controversial; although some studies have reported favorable survival associated with MSI EEC, other series did not find differences in grade, recurrence rate, and survival between MSI-positive and -negative EC [13].
Several studies have analyzed the morphological features associated with MSI, irrespective of the sporadic or hereditary nature of the tumors. MSI EEC tumors frequently have peritumoral lymphocytic infiltration and tumor-infiltrating lymphocytes (40/10 high-power fields), and some MSI ECs exhibit areas of dedifferentiation [21].
Alterations in the Phosphoinositide 3-Kinase (PI3K)/Akt Pathway
In EEC, the constitutive PI3K-AKT pathway is frequently activated in response to alterations of certain genes, such as those inactivating PTEN, mutations or amplifications of PIK3CA and somatic missense mutations within AKT kinases.
PTEN gene is located in 10q23, a region undergoing frequent somatic deletion in tumors. It encodes a 403-amino acid dual-specificity phosphatase containing a region of homology to tensin and auxilin, which are two cytoskeletal proteins. Among other activities, PTEN antagonizes the PI3K/AKT pathway, which results in downregulation of AKT phosphorylation activation. Thus, decreased expression of PTEN leads to increased levels of phospho-AKT, which results in both suppression of apoptosis and induction of cell cycle. PTEN is mutated in the germ line of patients with Cowden’s disease, a rare autosomal dominant cancer syndrome, which occasionally may be associated with EC. However, PTEN is also frequently somatically mutated in tumors from various tissues. PTEN may be also inactivated by deletion, as shown by the elevated frequency of loss of heterozygosity in different tumor types. Finally, a third proposed mechanism for PTEN inactivation is promoter hypermethylation. However, the true significance of PTEN promoter methylation is still under discussion.
Loss of heterozygosity at chromosome 10q23 occurs in 40 % of EECs [22]. Moreover, PTEN is the most frequently mutated gene in EEC (Fig. 2). The frequency of PTEN mutations in EEC varies between 24 and 50 % [2, 23,24,25] in different series, although one study has reported an incidence as high as 83 % [26]. In addition, PTEN silencing may occur not only in EEC and endometrial hyperplasia [25,26,27,28] but also in isolated glands in up to 40 % of premenopausal women [29], indicating a major role of this alteration in the initiation of some EEC.
PTEN mutations may occur throughout the entire coding region, but are more frequent in exons 5, 7, and 8. A high percentage of mutations in exon 5 (around 60 %) are single base substitution, being more common in codon 130 (Fig. 2). In contrast, frameshift mutations are more frequent in exons 7 and 8, where two hot spot deletions or insertions have been identified: two (A)6 sequences in codons 265–267 and codons 321–323. Mutations in those sites are characteristic of MSI tumors and suggest that some mutations in the PTEN gene are consequence of loss of DNA repair mechanism. Opinions differ, however, on the relationship between occurrence of PTEN gene mutations and the presence of MSI in EC. Thus, most series [24, 30, 31] have demonstrated that PTEN gene mutations occur more frequently in EC with MSI (65–86 %) than in those without it (20–36 %). However, other authors failed to find any relationship between high frequency of PTEN gene mutations and MSI in EC [26].
PTEN mutations have been detected more frequently in Caucasians relative to African-Americans, and have been correlated with young age, low FIGO-stage, low grade, and favorable prognosis in some studies [32,33,34]. However, other series have reported higher incidences of PTEN in advanced tumors (72 % of PTEN mutations in FIGO stage Ic as opposed to 56 % in FIGO stage Ia), as well as in less differentiated versus well-differentiated carcinomas (81 % in G2 vs. 44 % in G1 ECs) [35].
It has been suggested that PTEN immunostaining may be an effective method to screen for abnormal PTEN expression in tumors and premalignant lesions. However, some variability has been observed with different antibodies and techniques, particularly when correlating the immunohistochemical results with the presence of molecular alterations. Some studies have suggested that the monoclonal antibody 6.H2.1 is the only antibody that recognizes a pattern of PTEN expression that correlates with the presence of molecular alterations in PTEN (mutations, deletions, or promoter hypermethylation) [36, 37].
The PI3K pathway can be activated in EC not only by PTEN inactivating mutations but also by mutations in other genes. PI3K is a heterodimer composed of a catalytic subunit (p110α) encoded by PIK3CA, which is located at chromosome 3q26.32, and a regulatory subunit (p85α) encoded by PIK3R1. A high prevalence of mutations in the PIK3CA gene has been reported in EECs (up to 36 %) [2, 38,39,40,41,42,43], with most studies focusing on exons 9 and 20, as these two exons account for >80 % of mutations in other tumor types, and they encode the C-terminal helical and kinase domains of p110α [41, 42]. A significant association between PIK3CA and PTEN mutations has also been observed, suggesting an additive effect of these alterations in the activation of the PI3K/AKT pathway [41,42,43]. PIK3CA and KRAS mutations appear to be mutually exclusive [40, 43, 44]. However, their association with other genetic defects, such as CTNNB1 mutations or MSI, remains to be established [41, 42]. A link between PIK3CA mutations and adverse clinicopathologic parameters such as grade and stage has been described in some studies [42, 43]. Moreover, mutations in exon 20 are observed more frequently in high-grade than low-grade EECs (67 % vs. 33 %), while grade 1 ECCs are more frequently associated with exon 9 mutations (up to 57 %) [41]. PI3KCA amplification has also been reported in 12 % of EECs, occurring independently of mutational events at the same locus, and they are strongly associated with age, suggesting a role of PIK3CA amplification in the initiation and progress of ECs in older women [43].
More recently, mutations within the PI3K regulatory subunit (PIK3R1) have been reported in up to 43 % of EECs, preferentially localized in the p85α-iSH2 domain that mediates binding to p110α [2, 44]. These mutations are mutually exclusive with those affecting PIK3CA.
The AKT serine/threonine kinases regulate diverse cellular processes (survival, proliferation, invasion, and metabolism) and they are activated by direct recruitment to the plasma membrane via the pleckstrin homology (PH) domain. A missense mutation in the PH domain of AKT1 (E17K) previously described in other tumors [45], was demonstrated in 2 % of EECs [46]. Interestingly, the two tumors that displayed AKT1 mutations did not exhibit any mutations or LOH in PTEN, nor mutations in PIK3CA or KRAS. Subsequently, AKT1 mutations were demonstrated in 4–12 % of EECs [47, 48], while additional mutations in other AKT family members (AKT2 and AKT3) have been also described.
Alterations in the WNT Signaling Pathway
The Wnt signaling pathway plays an important role in normal and tumor cells. In the absence of an extracellular Wnt signal in normal cells, the free (cytoplasmic) β-catenin (coded by CTNNB1) level is low since the protein is targeted for destruction in the ubiquitin–proteasome system after phosphorylation by glycogen synthase kinase-3β(GSK-3β). The latter forms a complex with the adenomatous polyposis coli (APC) protein and other proteins, such as AXIN1, AXIN2, and protein phosphatase 2A. The most common molecular alterations in tumor cells leading to disruption of β-catenin degradation are mutations that inactivate APC or activate β-catenin itself. These alterations produce an accumulation of cytoplasmic β-catenin that translocates into the nucleus and, interacting with members of the lymphoid enhancer factor-1/T-cell factor (Lef-1/Tcf), activates transcription of various genes, such as CNDD1 and MYC.
Regarding EC, the Wnt signaling pathway is altered only in EEC. In these tumors, mutations of APC have not been detected [49, 50], but CTNNB1 mutations occurred in approximately 15–36 % of EEC (Fig. 3) [2, 49,50,51,52,53], and in 14 % of endometrial atypical hyperplasias [24]. Most mutations affect the aminoacids implicated in the downregulation of β-catenin through phosphorylation by this serine/threonine kinase (serine 33, serine 37, threonine 41, and serine 45) and two adjacent residues. Mutations in these residues render a fraction of cellular β-catenin insensitive to APC-mediated downregulation and are responsible for upregulation of cytoplasmic β-catenin and its accumulation in the nuclei of tumor cells, which can be detected by immunohistochemistry.
From a morphologic point of view, several studies have stressed the association between nuclear β-catenin accumulation and squamous metaplasia in EEC. Although nuclear β-catenin may be associated with usual squamous metaplasia, it is more characteristically associated with morular metaplasia and CTNNB1 mutations are found in 50 % of atypical endometrial hyperplasias with squamous morules [28] (Fig. 3).
Some series have not found significant relationship between CTNNB1 gene mutations and clinicopathologic features, such as age, tumor grade, and stage. However, in the TCGA series, CTNNB1 mutations were observed in 47 %, 36 %, and 17 % of grade 1, 2, and 3 EECs, respectively [2]. One study has shown an association with low-grade tumors and absence of lymph node metastases [53], suggesting that CTNNB1 mutations might occur in a subset of less aggressive ECs. In contrast, a recent study has found that CTNNB1 exon 3 mutations characterize an aggressive subset of low-grade and low-stage EEC occurring in younger women [52].
Mutations in SOX17 gene, which mediates proteasomal degradation of β-catenin, occur in 8 % EEC without MSI at recurrent positions (A96G and S403I) and are mutually exclusive with CTNNB1 mutations [2].
Alterations in the RAS-RAF-MEK-ERK Signaling Pathway
The RAS-RAF-MEK-ERK signaling pathway plays an important role in the development and progression of ECs. The RAS gene family consists of three closely related genes (KRAS, NRAS, and HRAS) that encode proteins with GTPase activity, which are localized at the inner plasma cellular membrane and involved in several signal transduction pathways.
KRAS mutations in codons 12 and 13 have been identified in 10–30 % of ECs (Fig. 2) [2, 50, 54,55,56]. Although some authors have failed to demonstrate a correlation between KRAS mutations and stage, grade, depth of invasion, age, or clinical outcome in EC, others have reported associations between KRAS mutations and presence of coexistent endometrial atypical hyperplasia, lymph node metastases, and clinical outcome in postmenopausal patients above 60 years [57]. An association between KRAS mutations and mucinous differentiation has also been reported [56, 58]. Several studies have tried to correlate KRAS mutations and MSI in EC, but results are contradictory.
Other RAS genes are infrequently mutated in EC. In the TCGA series, about 3 % of EECs carried point mutations at NRAS [2].
BRAF, which encodes a RAF family member that functions downstream of RAS, has been reported to be somatically mutated in a number of human cancers. Activating mutations of BRAF have been frequently observed in MSI colorectal carcinomas, in which mutations of BRAF and KRAS have been reported to be mutually exclusive [59]. Several series have analyzed the frequency of BRAF mutations in EC. Although one of these studies reported a 21 % incidence of BRAF mutations in EEC suggesting an association with MSI status [60], and another study reported 10 % of BRAF mutations in EEC [61], most studies have found a very low incidence of BRAF alterations [2, 62, 63], indicating a minor role of this gene in endometrial carcinogenesis.
In 10–12 % of EECs, somatic mutations in the tyrosine kinase receptor FGFR2 have been reported that are identical to the germline mutations associated with craniosynostosis and skeletal dysplasia syndromes [2, 64,65,66], the most common being S252W and N549K. FGFR2 mutations are associated with enhanced FGF signaling and downstream activity, predominantly through the RAS-MAPK pathway. Interestingly, while mutations in KRAS and FGFR2 are mutually exclusive events, FGFR2 and PTEN mutations frequently coexist [67].
ARID1A Gene Alterations
ARID1A is a recently identified tumor suppressor gene located at chromosome 1p36 that encodes a large nuclear protein (BAF 250A). This protein is a key component of the multi-protein SWI/SNF complex involved in chromatin remodeling that plays an integral role in controlling gene expression and regulating widely diverse cellular processes, from differentiation during development and proliferation, to DNA repair and tumor suppression [68, 69].
ARID1A mutations were recently described in ovarian clear cell carcinomas, 30 % of ovarian low-grade endometrioid carcinomas and in some cases of atypical endometriosis, a putative precursor of ovarian clear cell and endometrioid carcinomas, suggesting that ARID1A loss is a relatively specific event in the genesis of these tumors [70, 71]. Interestingly, most ARID1A mutations are insertion/deletion mutations, leading to generation of premature stop codons due to a frameshift, and giving rise to truncated proteins prone to degradation.
A number of studies have demonstrated that the loss of BAF250A protein is correlated with ARID1A mutation status [71, 72] (Fig. 4) and a high incidence of ARID1A mutations has been reported in both low-grade (up to 40 %) and high-grade (up to 60 %) EECs [73, 74]. Interestingly, in both grade 1 and grade 3 EECs, ARID1A mutations are significantly associated with concurrent mutations in PTEN and PIK3CA, suggesting a cooperative role of these pathways in EEC tumorigenesis [75]. In addition, ARID1A mutations seem to be mutually exclusive with TP53 mutations, but are associated with MSI [76, 77]. Interestingly, whereas near 75 % of sporadic EECs with MSI also carried ARID1A mutations, only 15 % of Lynch-associated EECs did, suggesting that ARIDIA is a causative gene instead of a target gene of MSI [77].
TP53 Gene Alterations
The TP53 tumor suppressor gene was initially identified as being essential for DNA damage checkpoint, but it was subsequently found to have a broader function after cellular stress, such as oncogene activation or hypoxia. The p53 protein is found at very low levels in normal cells. After stress, different pathways lead to posttranslational modification of the protein and its stabilization. This accumulation activates the transcription of a wide range of genes involved in various activities, including cell cycle inhibition and apoptosis depending on cellular context, extent of damage, or other unknown parameters.
Inactivation of TP53 is essentially due to small mutations (missense and nonsense mutations or insertions/deletions of several nucleotides), which lead to either expression of (90 %) or absence of expression (10 %) of the mutant protein. Thus, there is no a complete concordance between genotyping and immunohistochemistry in tumors with TP53 mutations. No inactivation of p53 gene expression by hypermethylation of transcription promoters has been demonstrated. In many instances, these mutations are associated with loss of the wild-type allele of the TP53 gene located on the short arm of chromosome 17.
TP53 mutations have been detected in approximately 10 % of EECs, being more frequent among grade 3 or advanced stage EECs [2, 78,80,81,82]. In contrast, 50–80 % of serous carcinomas carry TP53 mutations, more frequently associated with protein overexpression (Fig. 5) [2, 83, 84]. For this reason, p53 immunohistochemistry may help in the differential diagnosis of uterine serous carcinoma when it exhibits glands without papillary architecture from EEC [85] although it is important to note that EEC may have TP53 mutations.
TP53 mutation and expression have been reported to be an adverse prognostic factor in EC in some studies, but not in others. It has been proposed that the functional activity of mutant p53 protein is a strong predictor of survival in these patients [82]. Thus, the presence of dominant-negative p53 mutations, those that produce mutated proteins that complex with and inactivate wild-type protein, are associated with poor prognosis in advanced EEC.
One of the principal features of tumors with TP53 mutations is the high level of chromosomal instability that produces losses and gains that involve large chromosomal regions and specific genes. For this reason, serous carcinomas frequently carry amplification of genes like CCNE1, HER2, MYC, and PIK3CA [86, 87] (Table 2). Regarding HER2, although previous studies found inconsistencies regarding HER2 overexpression and amplification, the Gynaecological Oncology Group (GOG) phase II trial of trastuzumab in advanced and recurrent EC found that HER2 was amplified in 28 % of serous carcinomas as opposed to 7 % of EECs, demonstrating a correlation between HER2 overexpression and HER2 amplification [88]. However, no objective responses to trastuzumab therapy alone were reported in tumors displaying either HER2 overexpression or amplification. Marked heterogeneity of HER2 gene amplification has been described in endometrial serous carcinoma [89].
Cytogenetic Abnormalities
Cytogenetic studies have shown that most ECs have hyperdiploid karyotypes with relatively simple abnormalities, both numerical and structural, although cases also exist with complex chromosomal rearrangements [90]. Although aberrations of chromosome 1 leading to trisomy/tetrasomy 1q are the most frequent abnormalities reported, no specific karyotypic changes have been detected. A recent comparative genomic hybridization (CGH) study revealed more complex chromosomal imbalances in hormone-independent, type II ECs than in hormone-related, type I carcinomas. Moreover, the same study showed increased karyotypic complexity in relation to tumor grade in type I ECs, supporting the idea that tumor-phenotype is altered with accumulation of genomic imbalances [91]. Recently the same group compared DNA ploidy status with karyotypic and comparative genomic hybridization data on 51 ECs [92]. They found that gains of material from chromosomes 8 and 7 might be specifically correlated with DNA aneuploidy in ECs, The most frequent CGH findings in the DNA diploid tumors were gains of 1q and of parts of chromosome 10, suggesting that such gains could be an early event in ECs. In contrast, aberrations on chromosome 7 and 8 were rare in DNA diploid tumors but frequent in DNA aneuploid tumors. Of interest, none of the typical genes known to be altered in ECs, like PTEN, KRAS, and CTNNB1, are located on chromosomes 7 and 8.
Carcinosarcomas (Malignant Mixed Müllerian Tumors)
Molecular Abnormalities
A number of immunohistochemical and molecular studies support the monoclonal nature of uterine carcinosarcomas (CSs) [93]. For example, immunohistochemical studies have documented the expression of epithelial markers in the sarcomatous components of a large proportion of tumors. Moreover, X-chromosomal inactivation assays, mutational analyses, and LOH studies have all shown the carcinomatous and sarcomatous elements to share common genetic alterations [94, 95]. Provisional TCGA data (Tables 1 and 2) demonstrated a molecular profile more similar to serous than endometrioid carcinomas. However, a recent study including 17 uterine and 5 ovarian carcinosarcomas demonstrated that molecular alterations typical of EEC are also found in CSs. Thus, 40 % and 32 % of these tumors carried PTEN and ARID1A mutations respectively [96]. Mutations in PIK3CA are also frequent in uterine carcinosarcoma [96, 97]. More than 70 % of uterine CSs overexpressed EGFR, mainly in the sarcomatous component, but only about 20 % of them also carried EGFR amplification [97].
Uterine carcinosarcomas differ in their mutational profile from Müllerian adenosarcomas. These mixed tumors with a benign epithelial component frequently carry alterations of the PIK3CA/AKT/PTEN pathway (72 %), but infrequent TP53 mutations (17 %). In addition, the most frequent amplified genes in Müllerian adenosarcomas are CDK4 and MDM2 (28 %), and MYBL1 (22 %) if sarcomatous overgrowth is present [98].
Cytogenetic Abnormalities
It has been reported that karyotypes and CGH profiles of CSs are very similar to uterine carcinomas and different from sarcomas. Genetic imbalance profiles of CSs frequently mirror those of the epithelial component present in the tumor [91].
Uterine Sarcomas
Leiomyosarcoma
Molecular Abnormalities
Several series, including a relatively low number of tumors, have reported a 13–37 % frequency of TP53 mutations in these tumors [99,100,101]. PTEN mutational status has been studied in uterine sarcomas since these tumors frequently show loss of heterozygosity of 10q23.3 [102]; however, the incidence of PTEN mutations seems to be very low since only one mutation has been detected among 33 leiomyosarcomas analyzed in two different series [103, 104].
MED12 exon 2 mutations are frequently identified in uterine leiomyomas [105] but are mutually exclusive with uterine leiomyomas carrying a 12q14-15 (HMGA2) rearrangement [106]. However, MED12 mutation is a less frequently oncogenetic mechanism in uterine leiomyosarcoma and in extrauterine leiomyomas [107,108,109].
Cytogenetic Abnormalities
Most reported karyotypes in uterine leiomyosarcomas are complex without consistent numerical and structural aberrations (Table 3). In addition, CGH studies have confirmed a high frequency of gains and losses of several chromosomal regions [110]. This large number of nonrandom aberrations suggests that increased genetic instability plays a role in the origin of these tumors. The majority of molecular and cytogenetic data do not support an origin of leiomyosarcoma from its benign counterpart. A study of a series of smooth muscle tumors showed different gene expression profiles for leiomyosarcoma and leiomyoma [111]. However, MED12 mutation has been recently detected in a small subgroup of uterine leiomyosarcomas and in extrauterine leiomyomas [108, 109].
The transcriptional profile of a small group of cellular leiomyomas with a specific chromosome abnormality, e.g., del(1)(p11p36), is more similar to that seen in leiomyosarcoma than to profiles of normal myometrium and conventional leiomyoma [112]. A recent study demonstrated that 1p deletion occurs in approximately 25 % of cellular leiomyomas potentially associated with clinicopathologic features that are present with uterine sarcomas [113].
Several uterine smooth muscle proliferations, i.e., intravenous leiomyomatosis (IVL), disseminated peritoneal leiomyomatosis (DPL), and benign metastasizing leiomyoma (BML) are unusual because of their “aggressive” clinical behavior but they do not belong to the malignant category of smooth muscle tumors. However, several cytogenetic alterations have been detected that are worth discussing. A nonrandom pathogenetic event in IVL is the finding of a karyotype showing a der(14)t(12;14)(q15;q24) in addition to two normal copies of chromosome 12 (Table 3). The presence of t(12;14) in IVL, which is the most frequent abnormality in conventional leiomyomas, suggests a pathogenetic relationship between these two smooth muscle proliferations [114]. Recently an aCGH study in 9 IVL, reveled several losses and gains, including large deletions of 22q chromosome region in 6 [115]. Deletion at 22q is also a frequent aberration observed in BML by karyotyping [116] and aCGH [117]. Finally, DPL, a rare condition presenting with multiple benign smooth muscle proliferations throughout omental and peritoneal surfaces, has been suggested to have a common pathogenesis with conventional leiomyoma because of similar chromosome aberrations involving chromosomes 1, 3, 7, and 12 [118, 119].
Low-Grade Endometrial Stromal Sarcoma
Molecular Abnormalities
No mutations in TP53, PTEN, KRAS, or CTNNB1 have been described in low-grade endometrial stromal sarcomas (LG-ESS); however, nuclear β-catenin expression is seen in up to 40 % of these tumors [120]. This immunohistochemical pattern might be related to the downregulation of SFRP4, a negative modulator of the Wnt pathway [121].
Cytogenetic Abnormalities
Cytogenetic abnormalities reported in LG-ESSs demonstrate wide karyotypic heterogeneity. The most common abnormality is a t(7;17)(p15;q21) (Fig. 6a) resulting in the fusion of JAZF1 and SUZ12(JJAZ1) genes at 7p15 and 17q21, respectively [122]. JAZF1-SUZ12 fusion has been detected mostly in endometrial stromal nodules (~65 %), in ~48 % of low-grade (LG)-ESS and in ~12 % of undifferentiated ESSs [123, 124].
The second most frequent abnormality in these tumors is a t(6;7) (p21;p15) (Fig. 6b), a so-called variant translocation of the t(7;17), because of the involvement of 7p15 and 6p21 instead of the 17q21. [125]. At molecular level, this translocation resulted in a fusion gene between the PHD finger protein 1 (PHF1) gene, located in chromosome 6, band p21 and the JAZF1 at 7p15. Recently, the same authors expanded our knowledge of the 6p21 rearrangements in ESS. The PHF1 gene can fuse with JAZF1 at 7p15, with EPC1 at 10p11 and MEAF6 at 1p34 [126]. Moreover, it seems that there is a correlation in ESSs showing sex cord-like differentiation having PHF1 genetic rearrangement [127].
Two additional translocations have been described in ESSs, a t(X;22) (p11;q13) and t(X;17) (p11.2;q21.33) associated with a ZC3H7B-BCOR fusion and MBTD1-CXorf67 fusion, respectively [128, 129]. Gene expression profile showed that the t(X;17)/ZC3H7B-BCOR fusion clustered together with the t(7;17)/JAZF1-SUZ12.
Although endometrial stromal tumors are genetically heterogeneous, the different genes involved in stromal nodules and low-grade ESS are functionally related (PHF1, SUZ12, EPC1, MBTD1), being members of the polycomb gene family. Of interest, ZC3H7B-BCOR, MEAF6-PHF1, and EPC1-PHF1 fusions were also identify in ossifying fibromyxoid tumors [130] and JAZ1-PFH1 in an ossifying sarcoma of the heart [131].
High-Grade Endometrial Stromal Sarcomas
Cytogenetic Abnormalities
The most common cytogenetic alteration reported in high-grade ESS is a t(10;17)(q22;p13) associated with a YWHAE-NUTM2AB (aka FAM22A/B) fusion [132]. Tumors with YWHAE-NUTM2AB rearrangements constitute a distinct group of ESS, which is associated with small epithelioid cells, frequent necrosis, and more aggressive clinical behavior compared to JAZF1-LG-ESS but less aggressive than undifferentiated uterine sarcoma [133] (Fig. 6c). Thus, their distinction from undifferentiated uterine sarcoma is important for prognostic and therapeutic purposes, and standardized FISH analysis may be used in this setting [134, 135]. HG-ESSs with t(10;17) typically show strong and diffuse nuclear positivity for cyclinD1, Therefore, this can be used as a surrogate screening marker for these tumors [136]. Of interest, the same t(10;17)/YWHAE-NUTM2AB has been also reported in clear cell sarcoma, a subgroup of childhood renal tumors [137].
Other Sarcomas
Other sarcomas rarely occur in the uterus, e.g., embryonal rhabdomyosarcoma, primitive neuroectodermal tumor, or liposarcoma among others [138]. Inflammatory myofibroblastic tumors of the female genital tract are rare but characteristically show ALK rearrangement [139].
Conclusions
-
From a molecular point of view, endometrial cancer is classified into four groups: ultra-mutated, hypermutated, with low mutation frequency and microsatellite stable, and serous-like.
-
Ultra-mutated endometrial carcinoma is characterized by mutations in the exonuclease domain of POLE that produces an unusually high mutation rate.
-
Tumors with POLE mutations seem to have an excellent prognosis in spite of adverse molecular and pathological features.
-
The hypermutated endometrial carcinomas are tumors with microsatellite instability (MSI), most with MLH1 promoter methylation. Immunohistochemistry is a sensitive tool to detect MSI.
-
EC is the most common extracolonic tumor in patients with Lynch syndrome.
-
There are no differences in grade, recurrence rate, and survival between MSI-positive and -negative EC in most studies.
-
Most EECs are MSS EC with low mutation rate. In this group, the most frequently mutated genes are in the PI3K-AKT pathway (PTEN, PIK3CA, PIK3R1).
-
CTNNB1 mutations occur more frequently in grade 1 EEC and correlate with immunohistochemical nuclear expression of b-catenin. From a morphologic point of view, nuclear b-catenin accumulation is frequently seen in association with squamous morular metaplasia in EECs.
-
ARID1A mutations occur in 20–40 % of EEC depending on grade, are more frequent in MSI tumors, and are associated with BAF250A protein expression loss.
-
90 % of EC with extensive somatic copy number alterations and low mutation rates are serous carcinomas, although 10 % of high-grade EEC may have this molecular signature.
-
Genomic instability in serous carcinoma is secondary to p53 mutations.
-
HER-2 amplification/overexpression is more characteristic of serous carcinomas. However, overexpression of HER-2-neu is not a well-established prognostic marker in EC.
-
Molecular-genetic studies support the monoclonal nature of CSs, as they have shown that the carcinomatous and sarcomatous elements share common genetic alterations.
-
CSs more frequently have a molecular profile similar to serous carcinomas (TP53 mutations); however, up to 30–40 % have molecular alterations that are more typical of EEC (PTEN, ARID1A).
-
The most common chromosome translocations observed in LG-ESS are t(7;17)(p15;q21) associated with JAZF1-SUZ12 fusion, and translocation involving PHF1 gene at 6p21, which can frequently fuse with JAZF1 at 7p15, with EPC1 at 10p11 and MEAF6 at 1p34. Rarely, t(X;22) (p11;q13) and t(X;17) (p11.2;q21.33) associated with a ZC3H7B-BCOR fusion and MBTD1-CXorf67 fusion, respectively, can be also observed.
-
High-grade endometrial stromal sarcomas are characterized by the t(10;17)(q22;p13) associated with YWHAE-NUTM2AB.
References
Yeramian A, Moreno-Bueno G, Dolcet X, et al. Endometrial carcinoma: molecular alterations involved in tumor development and progression. Oncogene. 2013;32(4):403–13.
Cancer Genome Atlas Research Network, Kandoth C, Schultz N, Cherniack AD, et al. Integrated genomic characterization of endometrial carcinoma. Nature. 2013;497(7447):67–73.
Church DN, Stelloo E, Nout RA, et al. Prognostic significance of POLE proofreading mutations in endometrial cancer. J Natl Cancer Inst. 2014;107(1):402.
Hussein YR, Weigelt B, Levine DA, et al. Clinicopathological analysis of endometrial carcinomas harboring somatic POLE exonuclease domain mutations. Mod Pathol. 2015;28(4):505–14.
Meng B, Hoang LN, McIntyre JB, et al. POLE exonuclease domain mutation predicts long progression-free survival in grade 3 endometrioid carcinoma of the endometrium. Gynecol Oncol. 2014;134(1):15–9.
Billingsley CC, Cohn DE, Mutch DG, Stephens JA, Suarez AA, Goodfellow PJ. Polymerase ɛ (POLE) mutations in endometrial cancer: clinical outcomes and implications for Lynch syndrome testing. Cancer. 2015;121(3):386–94.
Haraldsdottir S, Hampel H, Tomsic J, et al. Colon and endometrial cancers with mismatch repair deficiency can arise from somatic, rather than germline, mutations. Gastroenterology. 2014;147(6):1308–1316.e1.
Boland CR, Thibodeau SN, Hamilton SR, et al. A National Cancer Institute Workshop on Microsatellite Instability for cancer detection and familial predisposition: development of international criteria for the determination of microsatellite instability in colorectal cancer. Cancer Res. 1998;58(22):5248–57.
Umar A, Boland CR, Terdiman JP, et al. Revised Bethesda Guidelines for hereditary nonpolyposis colorectal cancer (Lynch syndrome) and microsatellite instability. J Natl Cancer Inst. 2004;96(4):261–8.
Tafe LJ, Riggs ER, Tsongalis GJ. Lynch syndrome presenting as endometrial cancer. Clin Chem. 2014;60(1):111–21.
Vasen HF, Watson P, Mecklin JP, Lynch HT. New clinical criteria for hereditary nonpolyposis colorectal cancer (HNPCC, Lynch syndrome) proposed by the International Collaborative group on HNPCC. Gastroenterology. 1999;116(6):1453–6.
Wijnen J, de Leeuw W, Vasen H, et al. Familial endometrial cancer in female carriers of MSH6 germline mutations. Nat Genet. 1999;23(2):142–4.
Karamurzin Y, Rutgers JK. DNA mismatch repair deficiency in endometrial carcinoma. Int J Gynecol Pathol. 2009;28(3):239–55.
Esteller M, Catasus L, Matias-Guiu X, et al. hMLH1 promoter hypermethylation is an early event in human endometrial tumorigenesis. Am J Pathol. 1999;155(5):1767–72.
Kanaya T, Kyo S, Maida Y, et al. Frequent hypermethylation of MLH1 promoter in normal endometrium of patients with endometrial cancers. Oncogene. 2003;22(15):2352–60.
Hardisson D, Moreno-Bueno G, Sanchez L, et al. Tissue microarray immunohistochemical expression analysis of mismatch repair (hMLH1 and hMSH2 genes) in endometrial carcinoma and atypical endometrial hyperplasia: relationship with microsatellite instability. Mod Pathol. 2003;16(11):1148–58.
McConechy MK, Talhouk A, Li-Chang HH, et al. Detection of DNA mismatch repair (MMR) deficiencies by immunohistochemistry can effectively diagnose the microsatellite instability (MSI) phenotype in endometrial carcinomas. Gynecol Oncol. 2015; pii: S0090-8258(15)00584-3.
Schwartz S, Yamamoto H, Navarro M, Maestro M, Reventos J, Perucho M. Frameshift mutations at mononucleotide repeats in caspase-5 and other target genes in endometrial and gastrointestinal cancer of the microsatellite mutator phenotype. Cancer Res. 1999;59(12):2995–3002.
Catasus L, Matias-Guiu X, Machin P, et al. Frameshift mutations at coding mononucleotide repeat microsatellites in endometrial carcinoma with microsatellite instability. Cancer. 2000;88(10):2290–7.
Furlan D, Casati B, Cerutti R, et al. Genetic progression in sporadic endometrial and gastrointestinal cancers with high microsatellite instability. J Pathol. 2002;197(5):603–9.
Shia J, Black D, Hummer AJ, Boyd J, Soslow RA. Routinely assessed morphological features correlate with microsatellite instability status in endometrial cancer. Hum Pathol. 2008;39(1):116–25.
Peiffer SL, Herzog TJ, Tribune DJ, Mutch DG, Gersell DJ, Goodfellow PJ. Allelic loss of sequences from the long arm of chromosome 10 and replication errors in endometrial cancers. Cancer Res. 1995;55(9):1922–6.
Risinger JI, Hayes AK, Berchuck A, Barrett JC. PTEN/MMAC1 mutations in endometrial cancers. Cancer Res. 1997;57(21):4736–8.
Moreno-Bueno G, Hardisson D, Sarrio D, et al. Abnormalities of E- and P-cadherin and catenin (beta-, gamma-catenin, and p120ctn) expression in endometrial cancer and endometrial atypical hyperplasia. J Pathol. 2003;199(4):471–8.
Sun H, Enomoto T, Fujita M, et al. Mutational analysis of the PTEN gene in endometrial carcinoma and hyperplasia. Am J Clin Pathol. 2001;115(1):32–8.
Mutter GL, Lin MC, Fitzgerald JT, et al. Altered PTEN expression as a diagnostic marker for the earliest endometrial precancers. J Natl Cancer Inst. 2000;92(11):924–30.
Orbo A, Kaino T, Arnes M, Kopp M, Eklo K. Genetic derangements in the tumor suppressor gene PTEN in endometrial precancers as prognostic markers for cancer development: a population-based study from northern Norway with long-term follow-up. Gynecol Oncol. 2004;95(1):82–8.
Brachtel EF, Sanchez-Estevez C, Moreno-Bueno G, Prat J, Palacios J, Oliva E. Distinct molecular alterations in complex endometrial hyperplasia (CEH) with and without immature squamous metaplasia (squamous morules). Am J Surg Pathol. 2005;29(10):1322–9.
Mutter GL, Ince TA, Baak JP, Kust GA, Zhou XP, Eng C. Molecular identification of latent precancers in histologically normal endometrium. Cancer Res. 2001;61(11):4311–4.
Bussaglia E, del Rio E, Matias-Guiu X, Prat J. PTEN mutations in endometrial carcinomas: a molecular and clinicopathologic analysis of 38 cases. Hum Pathol. 2000;31(3):312–7.
Koul A, Willen R, Bendahl PO, Nilbert M, Borg A. Distinct sets of gene alterations in endometrial carcinoma implicate alternate modes of tumorigenesis. Cancer. 2002;94(9):2369–79.
Risinger JI, Hayes K, Maxwell GL, et al. PTEN mutation in endometrial cancers is associated with favorable clinical and pathologic characteristics. Clin Cancer Res. 1998;4(12):3005–10.
Maxwell GL, Risinger JI, Hayes KA, et al. Racial disparity in the frequency of PTEN mutations, but not microsatellite instability, in advanced endometrial cancers. Clin Cancer Res. 2000;6(8):2999–3005.
Salvesen HB, Stefansson I, Kretzschmar EI, et al. Significance of PTEN alterations in endometrial carcinoma: a population-based study of mutations, promoter methylation and PTEN protein expression. Int J Oncol. 2004;25(6):1615–23.
Konopka B, Paszko Z, Janiec-Jankowska A, Goluda M. Assessment of the quality and frequency of mutations occurrence in PTEN gene in endometrial carcinomas and hyperplasias. Cancer Lett. 2002;178(1):43–51.
Pallares J, Bussaglia E, Martinez-Guitarte JL, et al. Immunohistochemical analysis of PTEN in endometrial carcinoma: a tissue microarray study with a comparison of four commercial antibodies in correlation with molecular abnormalities. Mod Pathol. 2005;18(5):719–27.
Eritja N, Santacana M, Maiques O, Gonzalez-Tallada X, Dolcet X, Matias-Guiu X. Modeling glands with PTEN deficient cells and microscopic methods for assessing PTEN loss: endometrial cancer as a model. Methods. 2015;77–78:31–40.
Rudd ML, Price JC, Fogoros S, Godwin AK, Sgroi DC, Merino MJ, Bell DW. A unique spectrum of somatic PIK3CA (p110alpha) mutations within primary endometrial carcinomas. Clin Cancer Res. 2011;17(6):1331–40.
Oda K, Stokoe D, Taketani Y, McCormick F. High frequency of coexistent mutations of PIK3CA and PTEN genes in endometrial carcinoma. Cancer Res. 2005;65(23):10669–73.
Velasco A, Bussaglia E, Pallares J, et al. PIK3CA gene mutations in endometrial carcinoma: correlation with PTEN and K-RAS alterations. Hum Pathol. 2006;37(11):1465–72.
Catasus L, Gallardo A, Cuatrecasas M, Prat J. Concomitant PI3K-AKT and p53 alterations in endometrial carcinomas are associated with poor prognosis. Mod Pathol. 2009;22(4):522–9.
Kang S, Seo SS, Chang HJ, Yoo CW, Park SY, Dong SM. Mutual exclusiveness between PIK3CA and KRAS mutations in endometrial carcinoma. Int J Gynecol Cancer. 2008;18(6):1339–43.
Konopka B, Janiec-Jankowska A, Kwiatkowska E, et al. PIK3CA mutations and amplification in endometrioid endometrial carcinomas: relation to other genetic defects and clinicopathologic status of the tumors. Hum Pathol. 2011;42(11):1710–9.
Urick ME, Rudd ML, Godwin AK, Sgroi D, Merino M, Bell DW. PIK3R1 (p85alpha) is somatically mutated at high frequency in primary endometrial cancer. Cancer Res. 2011;71(12):4061–7.
Carpten JD, Faber AL, Horn C, et al. A transforming mutation in the pleckstrin homology domain of AKT1 in cancer. Nature. 2007;448(7152):439–44.
Shoji K, Oda K, Nakagawa S, et al. The oncogenic mutation in the pleckstrin homology domain of AKT1 in endometrial carcinomas. Br J Cancer. 2009;10(1):145–8.
Cohen Y, Shalmon B, Korach J, Barshack I, Fridman E, Rechavi G. AKT1 pleckstrin homology domain E17K activating mutation in endometrial carcinoma. Gynecol Oncol. 2010;116(1):88–91.
Dutt A, Salvesen HB, Greulich H, Sellers WR, Beroukhim R, Meyerson M. Somatic mutations are present in all members of the AKT family in endometrial carcinoma. Br J Cancer. 2009;101(7):1218–9.
Schlosshauer PW, Pirog EC, Levine RL, Ellenson LH. Mutational analysis of the CTNNB1 and APC genes in uterine endometrioid carcinoma. Mod Pathol. 2000;13(10):1066–71.
Moreno-Bueno G, Hardisson D, Sanchez C, et al. Abnormalities of the APC/beta-catenin pathway in endometrial cancer. Oncogene. 2002;21(52):7981–90.
Fukuchi T, Sakamoto M, Tsuda H, Maruyama K, Nozawa S, Hirohashi S. Beta-catenin mutation in carcinoma of the uterine endometrium. Cancer Res. 1998;58(16):3526–8.
Liu Y, Patel L, Mills GB, Lu KH, et al. Clinical significance of CTNNB1 mutation and Wnt pathway activation in endometrioid endometrial carcinoma. J Natl Cancer Inst. 2014;106(9). pii: dju245.
Saegusa M, Hashimura M, Yoshida T, Okayasu I. Beta-catenin mutations and aberrant nuclear expression during endometrial tumorigenesis. Br J Cancer. 2001;84(2):209–17.
Sasaki H, Nishii H, Takahashi H, et al. Mutation of the Ki-ras protooncogene in human endometrial hyperplasia and carcinoma. Cancer Res. 1993;53(8):1906–10.
Garcia-Dios DA, Lambrechts D, Coenegrachts L, et al. High-throughput interrogation of PIK3CA, PTEN, KRAS, FBXW7 and TP53 mutations in primary endometrial carcinoma. Gynecol Oncol. 2013;128(2):327–34.
Lagarda H, Catasus L, Arguelles R, Matias-Guiu X, Prat J. K-ras mutations in endometrial carcinomas with microsatellite instability. J Pathol. 2001;193(2):193–9.
Ito K, Watanabe K, Nasim S, et al. K-ras point mutations in endometrial carcinoma: effect on outcome is dependent on age of patient. Gynecol Oncol. 1996;63(2):238–46.
Alomari A, Abi-Raad R, Buza N, Hui P. Frequent KRAS mutation in complex mucinous epithelial lesions of the endometrium. Mod Pathol. 2014;27(5):675–80.
Rajagopalan H, Bardelli A, Lengauer C, Kinzler KW, Vogelstein B, Velculescu VE. Tumorigenesis: RAF/RAS oncogenes and mismatch-repair status. Nature. 2002;418(6901):934.
Feng YZ, Shiozawa T, Miyamoto T, et al. BRAF mutation in endometrial carcinoma and hyperplasia: correlation with KRAS and p53 mutations and mismatch repair protein expression. Clin Cancer Res. 2005;11(17):6133–8.
He M, Breese V, Hang S, Zhang C, Xiong J, Jackson C. BRAF V600E mutations in endometrial adenocarcinoma. Diagn Mol Pathol. 2013;22(1):35–40.
Salvesen HB, Kumar R, Stefansson I, et al. Low frequency of BRAF and CDKN2A mutations in endometrial cancer. Int J Cancer. 2005;115(6):930–4.
Pappa KI, Choleza M, Markaki S, et al. Consistent absence of BRAF mutations in cervical and endometrial cancer despite KRAS mutation status. Gynecol Oncol. 2006;100(3):596–600.
Byron SA, Gartside M, Powell MA, et al. FGFR2 point mutations in 466 endometrioid endometrial tumors: relationship with MSI, KRAS, PIK3CA, CTNNB1 mutations and clinicopathological features. PLoS One. 2012;7(2):e30801.
Gatius S, Velasco A, Azueta A, et al. FGFR2 alterations in endometrial carcinoma. Mod Pathol. 2011;24(11):1500–10.
Pollock PM, Gartside MG, Dejeza LC, et al. Frequent activating FGFR2 mutations in endometrial carcinomas parallel germline mutations associated with craniosynostosis and skeletal dysplasia syndromes. Oncogene. 2007;26(50):7158–62.
Byron SA, Gartside MG, Wellens CL, et al. Inhibition of activated fibroblast growth factor receptor 2 in endometrial cancer cells induces cell death despite PTEN abrogation. Cancer Res. 2008;68(17):6902–7.
Sif S, Saurin AJ, Imbalzano AN, Kingston RE. Purification and characterization of mSin3A-containing Brg1 and hBrm chromatin remodeling complexes. Genes Dev. 2001;15(5):603–18.
Reisman D, Glaros S, Thompson EA. The SWI/SNF complex and cancer. Oncogene. 2009;28(14):1653–68.
Jones S, Wang TL, Shih IM, et al. Frequent mutations of chromatin remodeling gene ARID1A in ovarian clear cell carcinoma. Science. 2010;330(6001):228–31.
Wiegand KC, Shah SP, Al-Agha OM, et al. ARID1A mutations in endometriosis-associated ovarian carcinomas. N Engl J Med. 2010;363(16):1532–43.
Maeda D, Mao TL, Fukayama M, Nakagawa S, et al. Clinicopathological significance of loss of ARID1A immunoreactivity in ovarian clear cell carcinoma. Int J Mol Sci. 2010;11(12):5120–8.
Guan B, Mao TL, Panuganti PK, et al. Mutation and loss of expression of ARID1A in uterine low-grade endometrioid carcinoma. Am J Surg Pathol. 2011;35(5):625–32.
Wiegand KC, Lee AF, Al-Agha OM, et al. Loss of BAF250a (ARID1A) is frequent in high-grade endometrial carcinomas. J Pathol. 2011;224(3):328–33.
McConechy MK, Ding J, Cheang MC, et al. Use of mutation profiles to refine the classification of endometrial carcinomas. J Pathol. 2012;228(1):20–30.
Allo G, Bernardini MQ, Wu RC, et al. ARID1A loss correlates with mismatch repair deficiency and intact p53 expression in high-grade endometrial carcinomas. Mod Pathol. 2014;27(2):255–61.
Bosse T, ter Haar NT, Seeber LM, et al. Loss of ARID1A expression and its relationship with PI3K-Akt pathway alterations, TP53 and microsatellite instability in endometrial cancer. Mod Pathol. 2013;26(11):1525–35.
Risinger JI, Dent GA, Ignar-Trowbridge D, et al. p53 gene mutations in human endometrial carcinoma. Mol Carcinog. 1992;5(4):250–3.
Enomoto T, Fujita M, Inoue M, et al. Alterations of the p53 tumor suppressor gene and its association with activation of the c-K-ras-2 protooncogene in premalignant and malignant lesions of the human uterine endometrium. Cancer Res. 1993;53(8):1883–8.
Kihana T, Hamada K, Inoue Y, et al. Mutation and allelic loss of the p53 gene in endometrial carcinoma. Incidence and outcome in 92 surgical patients. Cancer. 1995;76(1):72–8.
Swisher EM, Peiffer-Schneider S, Mutch DG, et al. Differences in patterns of TP53 and KRAS2 mutations in a large series of endometrial carcinomas with or without microsatellite instability. Cancer. 1999;85(1):119–26.
Sakuragi N, Watari H, Ebina Y, et al. Functional analysis of p53 gene and the prognostic impact of dominant-negative p53 mutation in endometrial cancer. Int J Cancer. 2005;116(4):514–9.
Tashiro H, Blazes MS, Wu R, et al. Mutations in PTEN are frequent in endometrial carcinoma but rare in other common gynecological malignancies. Cancer Res. 1997;57(18):3935–40.
Kovalev S, Marchenko ND, Gugliotta BG, Chalas E, Chumas J, Moll UM. Loss of p53 function in uterine papillary serous carcinoma. Hum Pathol. 1998;29(6):613–9.
Darvishian F, Hummer AJ, Thaler HT, et al. Serous endometrial cancers that mimic endometrioid adenocarcinomas: a clinicopathologic and immunohistochemical study of a group of problematic cases. Am J Surg Pathol. 2004;28(12):1568–78.
Le Gallo M, O'Hara AJ, Rudd ML, et al. Exome sequencing of serous endometrial tumors identifies recurrent somatic mutations in chromatin-remodeling and ubiquitin ligase complex genes. Nat Genet. 2012;44(12):1310–5.
Zhao S, Choi M, Overton JD, et al. Landscape of somatic single-nucleotide and copy-number mutations in uterine serous carcinoma. Proc Natl Acad Sci U S A. 2013;110(8):2916–21.
Fleming GF, Sill MW, Darcy KM, et al. Phase II trial of trastuzumab in women with advanced or recurrent, HER2-positive endometrial carcinoma: a Gynecologic Oncology Group study. Gynecol Oncol. 2010;116(1):15–20.
Buza N, English DP, Santin AD, Hui P. Toward standard HER2 testing of endometrial serous carcinoma: 4-year experience at a large academic center and recommendations for clinical practice. Mod Pathol. 2013;26(12):1605–12.
Mitelman F, Johansson B, Mertens F, editors. (2008). Mitelman database of chromosome aberrations in cancer. http://cgap.nci.nih.gov/Chromosomes/Mitelman.
Micci F, Teixeira MR, Haugom L, Kristensen G, Abeler VM, Heim S. Genomic aberrations in carcinomas of the uterine corpus. Genes Chromosomes Cancer. 2004;40(3):229–46.
Kildal W, Micci F, Risberg B, et al. Genomic imbalances in endometrial adenocarcinomas - comparison of DNA ploidy, karyotyping and comparative genomic hybridization. Mol Oncol. 2012;6(1):98–107.
Lopez-Garcia MA, Palacios J. Pathologic and molecular features of uterine carcinosarcomas. Semin Diagn Pathol. 2010;27(4):274–86.
Wada H, Enomoto T, Fujita M, et al. Molecular evidence that most but not all carcinosarcomas of the uterus are combination tumors. Cancer Res. 1997;57(23):5379–85.
Fujii H, Yoshida M, Gong ZX, et al. Frequent genetic heterogeneity in the clonal evolution of gynecological carcinosarcoma and its influence on phenotypic diversity. Cancer Res. 2000;60(1):114–20.
Jones S, Stransky N, McCord CL, et al. Genomic analyses of gynaecologic carcinosarcomas reveal frequent mutations in chromatin remodelling genes. Nat Commun. 2014;5:5006. doi:10.1038/ncomms6006.
Biscuola M, Van de Vijver K, Castilla MÁ, et al. Oncogene alterations in endometrial carcinosarcomas. Hum Pathol. 2013;44(5):852–9.
Howitt BE, Sholl LM, Dal Cin P, et al. Targeted genomic analysis of Müllerian adenosarcoma. J Pathol. 2015;235(1):37–49.
de Vos S, Wilczynski SP, Fleischhacker M, Koeffler P. p53 alterations in uterine leiomyosarcomas versus leiomyomas. Gynecol Oncol. 1994;54(2):205–8.
Jeffers MD, Farquharson MA, Richmond JA, McNicol AM. p53 immunoreactivity and mutation of the p53 gene in smooth muscle tumours of the uterine corpus. J Pathol. 1995;177(1):65–70.
Teneriello MG, Taylor RR, et al. Analysis of Ki-ras, p53, and MDM2 genes in uterine leiomyomas and leiomyosarcomas. Gynecol Oncol. 1997;65(2):330–5.
Quade BJ, Pinto AP, Howard DR, Peters 3rd WA, Crum CP. Frequent loss of heterozygosity for chromosome 10 in uterine leiomyosarcoma in contrast to leiomyoma. Am J Pathol. 1999;154(3):945–50.
Lancaster JM, Risinger JI, Carney ME, Barrett JC, Berchuck A. Mutational analysis of the PTEN gene in human uterine sarcomas. Am J Obstet Gynecol. 2001;184(6):1051–3.
Amant F, Vloeberghs V, Woestenborghs H, et al. ERBB-2 gene overexpression and amplification in uterine sarcomas. Gynecol Oncol. 2004;95(3):583–7.
Mehine M, Mäkinen N, Heinonen HR, Aaltonen LA, Vahteristo P. Genomics of uterine leiomyomas: insights from high-throughput sequencing. Fertil Steril. 2014;102(3):621–9.
Markowski DN, Bartnitzke S, Löning T, Drieschner N, Helmke BM, Bullerdiek J. MED12 mutations in uterine fibroids--their relationship to cytogenetic subgroups. Int J Cancer. 2012;131(7):1528–36.
Pérot G, Croce S, Ribeiro A, et al. MED12 alterations in both human benign and malignant uterine soft tissue tumors. PLoS One. 2012;7(6):e40015.
Ravegnini G, Mariño-Enriquez A, Slater J, et al. MED12 mutations in leiomyosarcoma and extrauterine leiomyoma. Mod Pathol. 2013;26(5):743–9.
Bertsch E, Qiang W, Zhang Q, et al. MED12 and HMGA2 mutations: two independent genetic events in uterine leiomyoma and leiomyosarcoma. Mod Pathol. 2014;27(8):1144–53.
Levy B, Mukherjee T, Hirschhorn K. Molecular cytogenetic analysis of uterine leiomyoma and leiomyosarcoma by comparative genomic hybridization. Cancer Genet Cytogenet. 2000;121(1):1–8.
Quade BJ, Wang TY, Sornberger K, Dal Cin P, Mutter GL, Morton CC. Molecular pathogenesis of uterine smooth muscle tumors from transcriptional profiling. Genes Chromosomes Cancer. 2004;40(2):97–108.
Christacos NC, Quade BJ, Dal Cin P, Morton CC. Uterine leiomyomata with deletions of Ip represent a distinct cytogenetic subgroup associated with unusual histologic features. Genes Chromosomes Cancer. 2006;45(3):304–12.
Hodge JC, Pearce KE, Clayton AC, Taran FA, Stewart EA. Uterine cellular leiomyomata with chromosome 1p deletions represent a distinct entity. Am J Obstet Gynecol. 2014; 210(6):572.e1–7.
Dal Cin P, Quade BJ, Neskey DM, Kleinman MS, Weremowicz S, Morton CC. Intravenous leiomyomatosis is characterized by a der(14)t(12;14)(q15;q24). Genes Chromosomes Cancer. 2003;36(2):205–6.
Buza N, Xu F, Wu W, Carr RJ, Li P, Hui P. Recurrent chromosomal aberrations in intravenous leiomyomatosis of the uterus: high-resolution array comparative genomic hybridization study. Hum Pathol. 2014;45(9):1885–92.
Nucci MR, Drapkin R, Dal Cin P, Fletcher CD, Fletcher JA. Distinctive cytogenetic profile in benign metastasizing leiomyoma: pathogenetic implications. Am J Surg Pathol. 2007;31(5):737–43.
Bowen JM, Cates JM, Kash S, et al. Genomic imbalances in benign metastasizing leiomyoma: characterization by conventional karyotypic, fluorescence in situ hybridization, and whole genome SNP array analysis. Cancer Genet. 2012;205(5):249–54.
Quade BJ, McLachlin CM, Soto-Wright V, Zuckerman J, Mutter GL, Morton CC. Disseminated peritoneal leiomyomatosis. Clonality analysis by X chromosome inactivation and cytogenetics of a clinically benign smooth muscle proliferation. Am J Pathol. 1997;150(6):2153–66.
Ordulu Z, Dal Cin P, Chong WW, et al. Disseminated peritoneal leiomyomatosis after laparoscopic supracervical hysterectomy with characteristic molecular cytogenetic findings of uterine leiomyoma. Genes Chromosomes Cancer. 2010;49(12):1152–60.
Ng TL, Gown AM, Barry TS, et al. Nuclear beta-catenin in mesenchymal tumors. Mod Pathol. 2005;18(1):68–74.
Hrzenjak A, Tippl M, Kremser ML, et al. Inverse correlation of secreted frizzled-related protein 4 and beta-catenin expression in endometrial stromal sarcomas. J Pathol. 2004;204(1):19–27.
Koontz JI, Soreng AL, Nucci M, et al. Frequent fusion of the JAZF1 and JJAZ1 genes in endometrial stromal tumors. Proc Natl Acad Sci U S A. 2001;98(11):6348–53.
Nucci MR, Harburger D, Koontz J, Dal Cin P, Sklar J. Molecular analysis of the JAZF1-JJAZ1 gene fusion by RT-PCR and fluorescence in situ hybridization in endometrial stromal neoplasms. Am J Surg Pathol. 2007;31(1):65–70.
Chiang S, Oliva E. Recent developments in uterine mesenchymal neoplasms. Histopathology. 2013;62(1):124–37.
Micci F, Walter CU, Teixeira MR, et al. Cytogenetic and molecular genetic analyses of endometrial stromal sarcoma: nonrandom involvement of chromosome arms 6p and 7p and confirmation of JAZF1/JJAZ1 gene fusion in t(7;17). Cancer Genet Cytogenet. 2003;144(2):119–24.
Micci F, Gorunova L, Gatius S, et al. MEAF6/PHF1 is a recurrent gene fusion in endometrial stromal sarcoma. Cancer Lett. 2014;347(1):75–8.
D'Angelo E, Ali RH, Espinosa I, Lee CH, Huntsman DG, Gilks B, Prat J. Endometrial stromal sarcomas with sex cord differentiation are associated with PHF1 rearrangement. Am J Surg Pathol. 2013;37(4):514–21.
Panagopoulos I, Thorsen J, Gorunova L, et al. Fusion of the ZC3H7B and BCOR genes in endometrial stromal sarcomas carrying an X;22-translocation. Genes Chromosomes Cancer. 2013;52(7):610–8.
Dewaele B, Przybyl J, Quattrone A, et al. Identification of a novel, recurrent MBTD1-CXorf67 fusion in low-grade endometrial stromal sarcoma. Int J Cancer. 2014;134(5):1112–22.
Antonescu CR, Sung YS, Chen CL, Zhang L, et al. Novel ZC3H7B-BCOR, MEAF6-PHF1, and EPC1-PHF1 fusions in ossifying fibromyxoid tumors--molecular characterization shows genetic overlap with endometrial stromal sarcoma. Genes Chromosomes Cancer. 2014;53(2):183–93.
Schoolmeester JK, Sukov WR, Maleszewski JJ, Bedroske PP, Folpe AL, Hodge JC. JAZF1 rearrangement in a mesenchymal tumor of nonendometrial stromal origin: report of an unusual ossifying sarcoma of the heart demonstrating JAZF1/PHF1 fusion. Am J Surg Pathol. 2013;37(6):938–42.
Lee CH, Ou W, Mariño-Enriquez A, Zhu M, et al. 14-3-3 Fusion oncogenes in high-grade endometrial stromal sarcoma. Proc Natl Acad Sci U S A. 2012;109:929–34.
Lee C-H, Mariño-Enriquez A, Ou W, et al. The clinicopathologic features of YWHAE-FAM22 endometrial stromal sarcomas – a histologically high-grade and clinically aggressive tumor. Am J Surg Pathol. 2012;36:641–53.
Stewart CJ, Leung YC, Murch A, Peverall J. Evaluation of fluorescence in-situ hybridization in monomorphic endometrial stromal neoplasms and their histological mimics: a review of 49 cases. Histopathology. 2014;65(4):473–82.
Sciallis AP, Bedroske PP, Schoolmeester JK, et al. High-grade endometrial stromal sarcomas: a clinicopathologic study of a group of tumors with heterogenous morphologic and genetic features. Am J Surg Pathol. 2014;38(9):1161–72.
Lee C-H, Ali RH, Rouzbahman M, Marino-Enriquez A, et al. Cyclin D1 as a diagnostic immunomarker for endometrial stromal sarcoma with YWHAE-FAM22 rearrangement. Am J Surg Pathol. 2012;36:641–53.
O'Meara E, Stack D, Lee CH, et al. Characterization of the chromosomal translocation t(10;17)(q22;p13) in clear cell sarcoma of kidney. J Pathol. 2012;227(1):72–80.
Oliva E. Cellular mesenchymal tumors of the uterus: a review emphasizing recent observations. Int J Gynecol Pathol. 2014;33(4):374–84.
Parra-Herran C, Quick CM, Howitt BE, Dal Cin PD, Quade BJ, Nucci MR. Inflammatory myofibroblastic tumor of the uterus: clinical and pathologic review of 10 cases including a subset with aggressive clinical course. Am J Surg Pathol. 2015;39(2):157–68.
Author information
Authors and Affiliations
Corresponding author
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2015 Springer International Publishing Switzerland
About this chapter
Cite this chapter
Palacios, J., Dal Cin, P. (2015). Molecular Pathology and Cytogenetics of Endometrial Carcinoma, Carcinosarcoma, and Uterine Sarcomas. In: Muggia, F., Santin, A.D., Oliva, E. (eds) Uterine Cancer. Current Clinical Oncology. Springer, Cham. https://doi.org/10.1007/7631_2015_6
Download citation
DOI: https://doi.org/10.1007/7631_2015_6
Publisher Name: Springer, Cham
Print ISBN: 978-3-319-47267-6
Online ISBN: 978-3-319-47269-0
eBook Packages: MedicineMedicine (R0)